Treatment of peripheral vascular disease using umbilical cord tissue-derived cells

ABSTRACT

Compositions and methods of using cells derived from umbilical cord tissue, to stimulate and support angiogenesis, to improve blood flow, to regenerate, repair, and improve skeletal muscle damaged by a peripheral ischemic event, and to protect skeletal muscle from ischemic damage in peripheral vascular disease patients are disclosed. In particular, methods of treating a patient having a peripheral vascular disease with umbilical derived cells and fibrin glue are disclosed.

CROSS-REFERENCE TO RELATED APPLICATIONS

This application is a continuation-in-part of U.S. patent applicationSer. No. 11/617,346, filed Dec. 28, 2006, which claims benefit to U.S.Provisional Patent Application No. 60/754,366, filed Dec. 28, 2005, thecontents of which are incorporated by reference herein, in theirentirety.

FIELD OF THE INVENTION

The invention relates to the field of cell based or regenerative therapyfor peripheral vascular disease patients, especially those withperipheral ischemia. In particular, the invention provides cells derivedfrom umbilical cord tissue having the capability to stimulate andsupport angiogenesis, to improve blood flow, to regenerate, repair, andimprove skeletal muscle damaged by a peripheral ischemic event, and toprotect skeletal muscle from ischemic damage.

BACKGROUND OF THE INVENTION

Various publications, including patents, published applications,technical articles and scholarly articles are cited throughout thespecification. Each of these cited publications is incorporated byreference herein, in its entirety.

Peripheral vascular disease (PVD) can result from atheroscleroticocclusion of the blood vessels, particularly in limbs and areas distalfrom the heart, resulting in diminished blood flow and insufficientoxygen perfusion to tissues in the vicinity of and downstream from theocclusion. PVD is frequently manifested in the iliac blood vessels,femoral and popliteal blood vessels, and subclavian blood vessels, andits effects can be exacerbated by thrombi, emboli, or trauma. It isestimated that approximately 8 to 12 million individuals in the UnitedStates, especially among the elderly population and those with diabetes,are afflicted with PVD.

Common symptoms of PVD include cramping in the upper and lower limbs andextremities, numbness, weakness, muscle fatigue, pain in the limbs andextremities, hypothermia in the limbs and extremities, discoloration ofthe extremities, dry or scaly skin, and hypertension. The most commonsymptom is claudication or feelings of pain, tightness, and fatigue inmuscles downstream of the occluded blood vessel that occurs during someform of exercise such as walking, but self-resolve after a period ofrest.

In terms of pathophysiology, the occluded blood vessels cause ischemiaof tissues at the site of and distal to the obstruction. This ischemiais generally referred to as peripheral ischemia, meaning that it occursin locations distal to the heart. The severity of the ischemia is afunction of the size and number of obstructions, whether the obstructionis near a muscle or organ, and whether there is sufficient redundantvasculature. In more severe cases, the ischemia results in death of theaffected tissues, and can result in amputation of affected limbs, oreven death of the patient.

Current methods for treatment of more severe cases of PVD includechemotherapeutic regimens, angioplasty, insertion of stents,reconstructive surgery, bypass grafts, resection of affected tissues, oramputation. Unfortunately, for many patients, such interventions showonly limited success, and many patients experience a worsening of theconditions or symptoms.

Presently, there is interest in using either stem cells, which candivide and differentiate, or muscles cells from other sources, includingsmooth and skeletal muscles cells, to assist the in the repair orreversal of tissue damage. Transplantation of stem cells can be utilizedas a clinical tool for reconstituting a target tissue, thereby restoringphysiologic and anatomic functionality. The application of stem celltechnology is wide-ranging, including tissue engineering, gene therapydelivery, and cell therapeutics, i.e., delivery of biotherapeutic agentsto a target location via exogenously supplied living cells or cellularcomponents that produce or contain those agents (For a review, seeTresco, P. A. et al., (2000) Advanced Drug Delivery Reviews 42:2-37).The identification of stem cells has stimulated research aimed at theselective generation of specific cell types for regenerative medicine.

One obstacle to realization of the therapeutic potential of stem celltechnology has been the difficulty of obtaining sufficient numbers ofstem cells. Embryonic, or fetal tissue, is one source of stem cells.Embryonic stem and progenitor cells have been isolated from a number ofmammalian species, including humans, and several such cell types havebeen shown capable of self-renewal and expansion, as welldifferentiation into a number of different cell lineages. But thederivation of stem cells from embryonic or fetal sources has raised manyethical and moral issues that are desirable to avoid by identifyingother sources of multipotent or pluripotent cells.

Postpartum tissues, such as the umbilical cord and placenta, havegenerated interest as an alternative source of stem cells. For example,methods for recovery of stem cells by perfusion of the placenta orcollection from umbilical cord blood or tissue have been described. Alimitation of stem cell procurement from these methods has been aninadequate volume of cord blood or quantity of cells obtained, as wellas heterogeneity in, or lack of characterization of, the populations ofcells obtained from those sources.

A reliable, well-characterized and plentiful supply of substantiallyhomogeneous populations of such cells having the ability todifferentiate into an array of skeletal muscle, pericyte, or vascularlineages would be an advantage in a variety of diagnostic andtherapeutic applications for skeletal muscle repair, regeneration, andimprovement, for the stimulation and/or support of angiogenesis, and forthe improvement of blood flow subsequent to a peripheral ischemic event,particularly in PVD patients.

SUMMARY OF THE INVENTION

One aspect of the invention features method of treating a patient havingperipheral vascular disease, the method comprising administering to thepatient umbilical cord tissue-derived cells in an amount effective totreat the peripheral vascular disease, wherein the umbilical cordtissue-derived cells are derived from human umbilical cord tissuesubstantially free of blood, wherein the cells are capable ofself-renewal and expansion in culture and have the potential todifferentiate into cells of at least a skeletal muscle, vascular smoothmuscle, pericyte, or vascular endothelium phenotype; wherein the cellsrequire L-valine for growth and can grow in at least about 5% oxygen;wherein the cells further comprise at least one of the followingcharacteristics: (a) potential for at least about 40 doublings inculture; (b) attachment and expansion on a coated or uncoated tissueculture vessel, wherein the coated tissue culture vessel comprises acoating of gelatin, laminin, collagen, polyornithine, vitronectin, orfibronectin; (c) production of at least one of tissue factor, vimentin,and alpha-smooth muscle actin; (d) production of at least one of CD10,CD13, CD44, CD73, CD90, PDGFr-alpha, PD-L2 and HLA-A,B,C; (e) lack ofproduction of at least one of CD31, CD34, CD45, CD80, CD86, CD117,CD141, CD178, B7-H2, HLA-G, and HLA-DR,DP,DQ, as detected by flowcytometry; (f) expression of a gene, which relative to a human cell thatis a fibroblast, a mesenchymal stem cell, or an iliac crest bone marrowcell, is increased for at least one of a gene encoding: interleukin 8;reticulon 1; chemokine (C-X-C motif) ligand 1 (melonoma growthstimulating activity, alpha); chemokine (C-X-C motif) ligand 6(granulocyte chemotactic protein 2); chemokine (C-X-C motif) ligand 3;tumor necrosis factor, alpha-induced protein 3; (g) expression of agene, which relative to a human cell that is a fibroblast, a mesenchymalstem cell, or an iliac crest bone marrow cell, is reduced for at leastone of a gene encoding: short stature homeobox 2; heat shock 27 kDaprotein 2; chemokine (C-X-C motif) ligand 12 (stromal cell-derivedfactor 1); elastin (supravalvular aortic stenosis, Williams-Beurensyndrome); Homo sapiens mRNA; cDNA DKFZp586M2022 (from cloneDKFZp586M2022); mesenchyme homeo box 2 (growth arrest-specific homeobox); sine oculis homeobox homolog 1 (Drosophila); crystallin, alpha B;disheveled associated activator of morphogenesis 2; DKFZP586B2420protein; similar to neuralin 1; tetranectin (plasminogen bindingprotein); src homology three (SH3) and cysteine rich domain; cholesterol25-hydroxylase; runt-related transcription factor 3; interleukin 11receptor, alpha; procollagen C-endopeptidase enhancer; frizzled homolog7 (Drosophila); hypothetical gene BC008967; collagen, type VIII, alpha1; tenascin C (hexabrachion); iroquois homeobox protein 5; hephaestin;integrin, beta 8; synaptic vesicle glycoprotein 2; neuroblastoma,suppression of tumorigenicity 1; insulin-like growth factor bindingprotein 2, 36 kDa; Homo sapiens cDNA FLJ12280 fis, clone MAMMA1001744;cytokine receptor-like factor 1; potassium intermediate/smallconductance calcium-activated channel, subfamily N, member 4; integrin,beta 7; transcriptional co-activator with PDZ-binding motif (TAZ); sineoculis homeobox homolog 2 (Drosophila); KIAA1034 protein;vesicle-associated membrane protein 5 (myobrevin); EGF-containingfibulin-like extracellular matrix protein 1; early growth response 3;distal-less homeo box 5; hypothetical protein FLJ20373; aldo-ketoreductase family 1, member C3 (3-alpha hydroxysteroid dehydrogenase,type II); biglycan; transcriptional co-activator with PDZ-binding motif(TAZ); fibronectin 1; proenkephalin; integrin, beta-like 1 (withEGF-like repeat domains); Homo sapiens mRNA full length insert cDNAclone EUROIMAGE 1968422; EphA3; KIAA0367 protein; natriuretic peptidereceptor C/guanylate cyclase C (atrionatriuretic peptide receptor C);hypothetical protein FLJ14054; Homo sapiens mRNA; cDNA DKFZp564B222(from clone DKFZp564B222); BCL2/adenovirus E1B 19 kDa interactingprotein 3-like; AE binding protein 1; cytochrome c oxidase subunit VIIapolypeptide 1 (muscle); similar to neuralin 1; B cell translocation gene1; hypothetical protein FLJ23191; and DKFZp586L151; (h) secretion of atleast one of MCP-1, IL-6, IL-8, GCP-2, HGF, KGF, FGF, HB-EGF, BDNF, TPO,MIP1b, RANTES, and TIMP1; and (i) lack of secretion of at least one ofTGF-beta2, ANG2, PDGFbb, MIP1a and VEGF, as detected by ELISA.

In a particular embodiment, the peripheral vascular disease isperipheral ischemia. In certain embodiments, the cells are induced invitro to differentiate into a skeletal muscle, vascular smooth muscle,pericyte, or vascular endothelium lineage cells prior to administration.In other embodiments, the cells are genetically engineered to produce agene product that promotes treatment of peripheral vascular disease.

In some embodiments of the method, cells are administered with at leastone other cell type, which may include skeletal muscle cells, skeletalmuscle progenitor cells, vascular smooth muscle cells, vascular smoothmuscle progenitor cells, pericytes, vascular endothelial cells, vascularendothelium progenitor cells, or other multipotent or pluripotent stemcells. The other cell type can administered simultaneously with, orbefore, or after, the umbilical cord tissue-derived cells.

In other embodiments, the cells are administered with at least one otheragent, which may be an antithrombogenic agent, an anti-inflammatoryagent, an immunosuppressive agent, an immunomodulatory agent,pro-angiogenic, or an antiapoptotic agent, for example. The other agentcan be administered simultaneously with, or before, or after, theumbilical cord tissue-derived cells.

The cells are preferably administered at or proximal to the sites of theperipheral ischemia, but can also be administered at sites distal to theperipheral ischemia. They can be administered by injection, infusion, adevice implanted in the patient, or by implantation of a matrix orscaffold containing the cells. The cells may exert a trophic effect,such as proliferation, on the skeletal muscle, vascular smooth muscle orvascular endothelium of the patient. The cells may induce migration ofskeletal muscle cells, vascular smooth muscle cells, vascularendothelial cells, skeletal muscle progenitor cells, pericytes, vascularsmooth muscle progenitor cells, or vascular endothelium progenitor cellsto the site or sites of peripheral vascular disease, such as peripheralischemia.

Another aspect of the invention features pharmaceutical compositions andkits for treating a patient having a peripheral vascular disease,comprising a pharmaceutically acceptable carrier and the umbilical cordtissue-derived cells described above or preparations made from suchumbilical cord tissue-derived cells. In some preferred embodiments, thepreparations comprise FGF and HGF. The pharmaceutical compositions andkits are designed and/or formulated for practicing the methods of theinvention as outlined above.

According to another aspect of the invention, the above-describedmethods may be practiced using a preparation made from the umbilicalcord tissue-derived cells, wherein the preparation comprises a celllysate of the umbilical cord tissue-derived cells, an extracellularmatrix of the umbilical cord tissue-derived cells or a conditionedmedium in which the umbilical cord tissue-derived cells were grown. Itis preferred that such preparations comprise FGF and HGF.

Other aspects of the invention feature pharmaceutical compositions andkits containing preparations comprising cell lysates, extracellularmatrices or conditioned media of the umbilical cord tissue-derivedcells.

One embodiment of the invention is a method of treating a patient havinga peripheral vascular disease, comprising administering a pharmaceuticalcomposition comprising a fibrin glue and an isolated homogenouspopulation of cells obtained from human umbilical cord tissue in anamount effective to treat the disease, wherein the umbilical cord tissueis substantially free of blood, and wherein isolated homogenouspopulation of cells is capable of self-renewal and expansion in culture,has the potential to differentiate and does not express CD117 and/ortelomerase. The isolated population of cells may also have one or moreof the following characteristics:

(a) expresses oxidized low density lipoprotein receptor 1, reticulon,chemokine receptor ligand 3, and/or granulocyte chemotactic protein;

(b) does not express CD31, CD34 or CD45;

(c) expresses, relative to a human fibroblast, mesenchymal stem cell, oriliac crest bone marrow cell, increased levels of interleukin 8 orreticulon 1;

(d) has the potential to differentiate into cells of at least a skeletalmuscle, vascular smooth muscle, pericyte or vascular endotheliumphenotype; and

(d) expresses CD10, CD13, CD44, CD73, and CD90.

In one embodiment, the peripheral vascular disease is peripheralischemia. The pharmaceutical composition is administered at the sites ofperipheral ischemia. In another embodiment, the pharmaceuticalcomposition is administered locally. In one embodiment, thepharmaceutical composition is administered by injection, infusion, adevice implanted in a patient, or by implantation of a matrix orscaffold containing the pharmaceutical composition. In an alternateembodiment, the pharmaceutical composition is administered byintramuscular injection and injection into adipose depots in muscle. Inanother embodiment, the pharmaceutical composition is administered byinjection into interstitial spaces so as not to enter directly intocirculation. The isolated population of cells may be induced in vitro todifferentiate into a skeletal muscle, vascular muscle, pericyte orvascular endothelium lineage prior to administration. The population ofcells may also be genetically engineered to produce a gene product thatpromotes treatment of peripheral vascular disease. Optionally, thecomposition further comprises an agent selected from the groupconsisting of an antithrombogenic agent, an immunosuppressive agent, animmunomodulatory agent, a pro-angiogenic, an antiapoptotic agent andmixtures thereof. Alternatively, the composition further comprises atleast one other cell type (such as e.g. a skeletal muscle cell, askeletal muscle progenitor cell, a vascular smooth muscle cell, avascular smooth muscle progenitor cell, a pericyte, a vascularendothelial cell, a vascular endothelium progenitor cell or othermultipotent or pluripotent stem cell). In one embodiment, thepharmaceutical composition exerts a trophic effect (such as e.g.proliferation of vascular endothelial cells). In another embodiment, thepharmaceutical composition induces migration of vascular endothelialcells and/or vascular endothelium progenitor cells to the sites of theperipheral disease. In yet an alternate embodiment, the pharmaceuticalcomposition induces migration of vascular smooth muscle cells and/orvascular smooth muscle progenitor cells to the sites of the peripheraldisease. In another embodiment, the pharmaceutical composition inducesmigration of pericytes to the sites of the peripheral vascular disease.In one embodiment, the fibrin glue comprises fibrinogen and thrombin. Inanother embodiment, the fibrin glue comprises from about 16 to about 24IU/ml of thrombin and from about 39.3 to about 60.7 mg/ml of fibrinogen.

Another embodiment of the invention is a method of treating a patienthaving a peripheral vascular disease, comprising administering a fibringlue (e.g. a composition comprising fibrinogen and thrombin) and anisolated homogenous population of cells obtained from human umbilicalcord tissue in an amount effective to treat the disease, wherein theumbilical cord tissue is substantially free of blood, and whereinisolated homogenous population of the cells is capable of self-renewaland expansion in culture, has the potential to differentiate and doesnot express CD117 and/or telomerase. The isolated population of cellsmay have other characteristics, including one or more of the following:

(a) expresses oxidized low density lipoprotein receptor 1, reticulon,chemokine receptor ligand 3, and/or granulocyte chemotactic protein;

(b) does not express CD31, CD34 or CD45;

(c) express, relative to a human fibroblast, mesenchymal stem cell, oriliac crest bone marrow cell, increased levels of interleukin 8 orreticulon 1;

(d) has the potential to differentiate into cells of at least a skeletalmuscle, vascular smooth muscle, pericyte or vascular endotheliumphenotype; and

(d) expresses CD10, CD13, CD44, CD73, and CD90.

In one embodiment, the peripheral vascular disease is peripheralischemia and, optionally, the fibrin glue and the population of cellsare administered at the sites of peripheral ischemia. Various routes ofadministration may be used including administered by injection,infusion, a device implanted in a patient, or by implantation of amatrix or scaffold containing the cells. In one embodiment, thepopulation of cells and fibrin glue are administered locally (such ase.g. by intramuscular injection and injection into adipose depots inmuscle). In another embodiment, the cells and fibrin glue areadministered by injection into interstitial spaces so as not to directlyenter into circulation. Optionally, the isolated population of cells isinduced in vitro to differentiate into a skeletal muscle, vascularmuscle, pericyte or vascular endothelium lineage prior toadministration. The population of cells may also be geneticallyengineered to produce a gene product that promotes treatment ofperipheral vascular disease. In one embodiment, the method furthercomprises administration of an agent selected from the group consistingof an antithrombogenic agent, an immunosuppressive agent, animmunomodulatory agent, a pro-angiogenic, an antiapoptotic agent andmixtures thereof. In another embodiment, the method further comprisesadministration of at least one other cell type (such as e.g. a skeletalmuscle cell, a skeletal muscle progenitor cell, a vascular smooth musclecell, a vascular smooth muscle progenitor cell, a pericyte, a vascularendothelial cell, a vascular endothelium progenitor cell or othermultipotent or pluripotent stem cell). In one embodiment, the populationof cells exerts a trophic effect (e.g. proliferation of vascularendothelial cells). The population of cells may induce migration ofvascular endothelial cells and/or vascular endothelium progenitor cellsto the sites of the peripheral disease. Alternatively, the population ofcells may induce migration of vascular smooth muscle cells and/orvascular smooth muscle progenitor cells to the sites of the peripheraldisease. The population of cells also may induce migration of pericytesto the sites of the peripheral vascular disease. The fibrin glue maycomprise fibrinogen and thrombin. In one embodiment, the fibrin glue isadministered simultaneously with, or before, or after, the isolatedhomogenous population of cells obtained from human umbilical cordtissue. In another embodiment, the fibrin glue comprises from about 16to about 24 IU/ml of thrombin and from about 39.3 to about 60.7 mg/ml offibrinogen.

Another embodiment of the invention is a kit for treating a patienthaving a peripheral vascular disease comprising fibrinogen, thrombin andan isolated homogenous population of cells obtained from human umbilicalcord tissue in an amount effective to treat the disease, wherein theumbilical cord tissue is substantially free of blood, and wherein saidisolated homogenous population of the cells is capable of self-renewaland expansion in culture, has the potential to differentiate and do notexpress CD117 and/or telomerase. The kit may further compriseinstructions for use. In one embodiment, the fibrinogen and isolatedhomogenous population of cells are in provided in a composition to whichthrombin may be added immediately prior to use. The isolated populationof cells may have other characteristics, including one or more of thefollowing:

(a) expresses oxidized low density lipoprotein receptor 1, reticulon,chemokine receptor ligand 3, and/or granulocyte chemotactic protein;

(b) does not express CD31, CD34 or CD45;

(c) express, relative to a human fibroblast, mesenchymal stem cell, oriliac crest bone marrow cell, increased levels of interleukin 8 orreticulon 1;

(d) has the potential to differentiate into cells of at least a skeletalmuscle, vascular smooth muscle, pericyte or vascular endotheliumphenotype; and

(d) expresses CD10, CD13, CD44, CD73, and CD90.

In one embodiment, the kit comprises from about 16 to about 24 IU/ml ofthrombin and from about 39.3 to about 60.7 mg/ml of fibrinogen. In oneembodiment, the kit comprises a fibrinogen component comprising fibrinand factor XII and a thrombin component comprising thrombin and calcium.

Other features and advantages of the invention will be understood byreference to the detailed description and examples that follow.

BRIEF DESCRIPTION OF THE DRAWINGS

FIG. 1 shows the effect of hUTC lot#120304, MSCs, and fibroblasts on theproliferation of endothelial cells. Endothelial cells were seeded ontothe bottom of a 24-well tissue culture dish at a density of 5000cells/cm² (10,000 cells/well) and hUTC lot#120304, MSCs, or fibroblastsinside transwell inserts at a density of 5000 cells/cm² (1,650cells/insert) in co-culture media (Hayflick 80%+EGM-2MV 20% or Hayflick50%+EGM-2MV 50%). After 7 days of co-culture, cells were harvested andcounted using a Guava® instrument. Endothelial cells were alsomaintained in EGM-2MV media as positive control. A, HUVECs. B, HCAECs.C, HIAECs.

FIG. 2 shows the effect of hUTC lot#120304 and neutralizing antibodieson the proliferation of endothelial cells. HUVECs or HCAECs were seededonto the bottom of a 24-well tissue culture dish at a density of 5000cells/cm² (10,000 cells/well) and hUTC lot#120304 inside transwellinserts at a density of 5000 cells/cm² (1,650 cells/insert) inco-culture media (Hayflick 50%+EGM-2MV 50%). Neutralizing antibodies toFGF (7 μg/ml), HGF (1 μg/ml), or VEGF (1 μg/ml) were also added at thistime. After 7 days of co-culture, cells were harvested and counted usinga Guava® instrument. Endothelial cells were also maintained in EGM-2MVmedia as positive control. Cells treated with growth factor alone andgrowth factor plus neutralizing antibodies are shown. A and B, HUVECs. Cand D, HCAECs.

FIG. 3 shows the effect of hUTC lot#120304 cell lysate and neutralizingantibodies on proliferation of HUVECs. HUVECs were seeded onto thebottom of a 24-well tissue culture dish at a density of 5000 cells/cm²(10,000 cells/well) in EGM-2MV media for 8 h. Cells were thenserum-starved by overnight incubation in 0.5 ml of EGM-2MV mediacontaining 0.5% FBS and without growth factors. Afterwards, FBS, freshlyprepared hUTC lot#120304 cell lysates, and neutralizing antibodies toFGF (7 μg/ml) or HGF (1 μg/ml) were added. After 4 days of culture,cells were harvested and counted using a Guava® instrument. Light greybars, media controls. Medium grey bars, HUVECs incubated with lysatecontaining 62.5 μg of protein. Dark grey bars, HUVECs incubated withlysate containing 125 μg of protein.

FIG. 4 shows the effect of hUTCs and MSCs on the migration ofendothelial cells. HUVECs or HCAECs were seeded inside transwell insertsat a density of 5000 cells/cm² (23,000 cells/insert) and hUTC lot#120304or MSCs onto the bottom of a E-well tissue culture dish at a density of5000 cells/cm² (48,000 cells/well) in co-culture media (Hayflick50%+EGM-2MV 50%). After 7 days of co-culture, cells that were on theunderside of the transwell insert were harvested and counted using aGuava® instrument. Endothelial cells were also maintained in EGM-2MVmedia as control. A, HUVECs. B, HCAECs.

FIG. 5 shows the effect of hUTC lot#120304 and neutralizing antibodieson the migration of endothelial cells. HUVECs or HCAECs were seededinside transwell inserts at a density of 5000 cells/cm² (23,000cells/insert) and hUTC lot#120304 onto the bottom of a 6-well tissueculture dish at a density of 5000 cells/cm² (48,000 cells/well) inco-culture media (Hayflick 50%+EGM-2MV 50%). Neutralizing antibodies toFGF (7 ng/ml) or HGF (1 ng/ml) were added at this time. After 7 days ofco-culture, cells that were on the underside of the transwell insertwere harvested and counted using a Guava® instrument. Endothelial cellswere also maintained in EGM-2MV media as control. A, HUVECs. B, HCAECs.

FIG. 6 shows the laser doppler perfusion data from the experiment withNSG mice for the study disclosed in Example 5. Data are expressed asmean±sem. The identity of data points is displayed in the legend.Numbers in parentheses are (1) P<0.001 compared to appropriate control;(2) P<0.05 compared to hUTC cells without fibrin.

FIG. 7 shows the laser doppler perfusion data from the experiment withnude mice for the study disclosed in Example 5. Data are expressed asmean±sem. The identity of data points is displayed in the legend.Numbers in parentheses are (1) P<0.001 compared to appropriate control;(2) P<0.05 compared to hUTC cells without fibrin.

FIG. 8 shows laser doppler perfusion data comparing systemic (IV), local(IM), and local+fibrin glue delivery for the study disclosed in Example6. Data are expressed as mean±sem.

FIG. 9 shows laser doppler perfusion data showing different doses ofhUTC in fibrin glue delivered locally (IM) for the study disclosed inExample 6. Data are expressed as mean±sem.

FIG. 10 shows laser doppler perfusion data comparing systemic (IV),local (IM), and local+fibrin glue delivery at 14 days post-injury forthe study disclosed in Example 6. Data shown as mean for clarity.

FIG. 11 shows laser doppler perfusion for the study disclosed in Example7. The identity of data points is displayed in the legend. *, P<0.05;***, P<0.001.

FIG. 12 shows capillary density of ischemic limbs compared tonon-ischemic limbs of mice surviving to 21 days for the study disclosedin Example 7.

FIG. 13 shows arteriole density ischemic limbs compared to non-ischemiclimbs of mice surviving to 21 days for the study disclosed in Example 7.

DETAILED DESCRIPTION

Various terms are used throughout the specification and claims. Suchterms are to be given their ordinary meaning in the art unless otherwiseindicated. Other specifically defined terms are to be construed in amanner consistent with the definition provided herein.

Stem cells are undifferentiated cells defined by the ability of a singlecell both to self-renew and to differentiate to produce progeny cells,including self-renewing progenitors, non-renewing progenitors, andterminally differentiated cells. Stem cells are also characterized bytheir ability to differentiate in vitro into functional cells of variouscell lineages from multiple germ layers (endoderm, mesoderm andectoderm), as well as to give rise to tissues of multiple germ layersfollowing transplantation, and to contribute substantially to most, ifnot all, tissues following injection into blastocysts.

Stem cells are classified according to their developmental potential as:(1) totipotent; (2) pluripotent; (3) multipotent; (4) oligopotent; and(5) unipotent. Totipotent cells are able to give rise to all embryonicand extraembryonic cell types. Pluripotent cells are able to give riseto all embryonic cell types. Mutt/potent cells include those able togive rise to a subset of cell lineages, but all within a particulartissue, organ, or physiological system. For example, hematopoietic stemcells (HSC) can produce progeny that include HSC (self-renewal), bloodcell-restricted oligopotent progenitors, and all cell types and elements(e.g., platelets) that are normal components of the blood. Cells thatare oligopotent can give rise to a more restricted subset of celllineages than multipotent stem cells. Cells that are unipotent are ableto give rise to a single cell lineage (e.g., spermatogenic stem cells).

Stem cells are also categorized on the basis of the source from whichthey are obtained. An adult stem cell is generally a multipotentundifferentiated cell found in tissue comprising multiple differentiatedcell types. The adult stem cell can renew itself. Under normalcircumstances, it can also differentiate to yield the specialized celltypes of the tissue from which it originated, and possibly other tissuetypes. An embryonic stem cell is a pluripotent cell from the inner cellmass of a blastocyst-stage embryo. A fetal stem cell is one thatoriginates from fetal tissues or membranes. A postpartum stem cell is amultipotent or pluripotent cell that originates substantially fromextraembryonic tissue available after birth, namely, the placenta andthe umbilical cord. These cells have been found to possess featurescharacteristic of pluripotent stem cells, including rapid proliferationand the potential for differentiation into many cell lineages.Postpartum stem cells may be blood-derived (e.g., as are those obtainedfrom umbilical cord blood) or non-blood-derived (e.g., as obtained fromthe non-blood tissues of the umbilical cord and placenta).

Embryonic tissue is typically defined as tissue originating from theembryo (which in humans refers to the period from fertilization to aboutsix weeks of development. Fetal tissue refers to tissue originating fromthe fetus, which in humans refers to the period from about six weeks ofdevelopment to parturition. Extraembryonic tissue is tissue associatedwith, but not originating from, the embryo or fetus. Extraembryonictissues include extraembryonic membranes (chorion, amnion, yolk sac andallantois), umbilical cord and placenta (which itself forms from thechorion and the maternal decidua basalis).

Differentiation is the process by which an unspecialized (“uncommitted”)or less specialized cell acquires the features of a specialized cell,such as a nerve cell or a muscle cell, for example. A differentiatedcell is one that has taken on a more specialized (“committed”) positionwithin the lineage of a cell. The term committed, when applied to theprocess of differentiation, refers to a cell that has proceeded in thedifferentiation pathway to a point where, under normal circumstances, itwill continue to differentiate into a specific cell type or subset ofcell types, and cannot, under normal circumstances, differentiate into adifferent cell type or revert to a less differentiated cell type.De-differentiation refers to the process by which a cell reverts to aless specialized (or committed) position within the lineage of a cell.As used herein, the lineage of a cell defines the heredity of the cell,i.e. which cells it came from and what cells it can give rise to. Thelineage of a cell places the cell within a hereditary scheme ofdevelopment and differentiation.

In a broad sense, a progenitor cell is a cell that has the capacity tocreate progeny that are more differentiated than itself, and yet retainsthe capacity to replenish the pool of progenitors. By that definition,stem cells themselves are also progenitor cells, as are the moreimmediate precursors to terminally differentiated cells. When referringto the cells of the present invention, as described in greater detailbelow, this broad definition of progenitor cell may be used. In anarrower sense, a progenitor cell is often defined as a cell that isintermediate in the differentiation pathway, i.e., it arises from a stemcell and is intermediate in the production of a mature cell type orsubset of cell types. This type of progenitor cell is generally not ableto self-renew. Accordingly, if this type of cell is referred to herein,it will be referred to as a non-renewing progenitor cell or as anintermediate progenitor or precursor cell.

As used herein, the phrase differentiates into a mesodermal, ectodermalor endodermal lineage refers to a cell that becomes committed to aspecific mesodermal, ectodermal or endodermal lineage, respectively.Examples of cells that differentiate into a mesodermal lineage or giverise to specific mesodermal cells include, but are not limited to, cellsthat are adipogenic, chondrogenic, cardiogenic, dermatogenic,hematopoietic, hemangiogenic, myogenic, nephrogenic, urogenitogenic,osteogenic, pericardiogenic, or stromal. Examples of cells thatdifferentiate into ectodermal lineage include, but are not limited toepidermal cells, neurogenic cells, and neurogliagenic cells. Examples ofcells that differentiate into endodermal lineage include, but are notlimited to, pleurigenic cells, hepatogenic cells, cells that give riseto the lining of the intestine, and cells that give rise to pancreogenicand splanchogenic cells.

The cells used in the present invention are generally referred to asreferred to as umbilical cord tissue-derived cells (UTC(s) or hUTC(s)).They also may sometimes be referred to as umbilicus-derived cells(UDCs). In addition, the cells may be described as being stem orprogenitor cells, the latter term being used in the broad sense. Theterm derived is used to indicate that the cells have been obtained fromtheir biological source and grown or otherwise manipulated in vitro(e.g., cultured in a Growth Medium to expand the population and/or toproduce a cell line). The in vitro manipulations of umbilical stem cellsand the unique features of the umbilicus-derived cells of the presentinvention are described in detail below.

Pericytes, also known in the art as Rouget cells or mural cells, refersto the cells typically found embedded within the vascular basementmembrane of blood microvessels (Armulik A et al. (2005) Circ. Res.97:512-23), that are believed to play a role in, among other things,communication/signalling with endothelial cells, vasoconstriction,vasodilation, the regulation of blood flow, blood vasculature formationand development, angiogenesis, and endothelial differentiation andgrowth arrest (Bergers G et al. (2005) Neuro-Oncology 7:452-64).

Various terms are used to describe cells in culture. Cell culture refersgenerally to cells taken from a living organism and grown undercontrolled condition (“in culture” or “cultured”). A primary cellculture is a culture of cells, tissues, or organs taken directly from anorganism(s) before the first subculture. Cells are expanded in culturewhen they are placed in a Growth Medium under conditions that facilitatecell growth and/or division, resulting in a larger population of thecells. When cells are expanded in culture, the rate of cellproliferation is sometimes measured by the amount of time needed for thecells to double in number. This is referred to as doubling time.

A cell line is a population of cells formed by one or moresubcultivations of a primary cell culture. Each round of subculturing isreferred to as a passage. When cells are subcultured, they are referredto as having been passaged. A specific population of cells, or a cellline, is sometimes referred to or characterized by the number of timesit has been passaged. For example, a cultured cell population that hasbeen passaged ten times may be referred to as a P10 culture. The primaryculture, i.e., the first culture following the isolation of cells fromtissue, is designated P0. Following the first subculture, the cells aredescribed as a secondary culture (P1 or passage 1). After the secondsubculture, the cells become a tertiary culture (P2 or passage 2), andso on. It will be understood by those of skill in the art that there maybe many population doublings during the period of passaging; thereforethe number of population doublings of a culture is greater than thepassage number. The expansion of cells (i.e., the number of populationdoublings) during the period between passaging depends on many factors,including but not limited to the seeding density, substrate, medium,growth conditions, and time between passaging.

A conditioned medium is a medium in which a specific cell or populationof cells has been cultured, and then removed. When cells are cultured ina medium, they may secrete cellular factors that can provide trophicsupport to other cells. Such trophic factors include, but are notlimited to hormones, cytokines, extracellular matrix (ECM), proteins,vesicles, antibodies, and granules. The medium containing the cellularfactors is the conditioned medium.

Generally, a trophic factor is defined as a substance that promotessurvival, growth, proliferation and/or maturation of a cell, orstimulates increased activity of a cell.

When referring to cultured vertebrate cells, the term senescence (alsoreplicative senescence or cellular senescence) refers to a propertyattributable to finite cell cultures; namely, their inability to growbeyond a finite number of population doublings (sometimes referred to asHayflick's limit). Although cellular senescence was first describedusing fibroblast-like cells, most normal human cell types that can begrown successfully in culture undergo cellular senescence. The in vitrolifespan of different cell types varies, but the maximum lifespan istypically fewer than 100 population doublings (this is the number ofdoublings for all the cells in the culture to become senescent and thusrender the culture unable to divide). Senescence does not depend onchronological time, but rather is measured by the number of celldivisions, or population doublings, the culture has undergone. Thus,cells made quiescent by removing essential growth factors are able toresume growth and division when the growth factors are re-introduced,and thereafter carry out the same number of doublings as equivalentcells grown continuously. Similarly, when cells are frozen in liquidnitrogen after various numbers of population doublings and then thawedand cultured, they undergo substantially the same number of doublings ascells maintained unfrozen in culture. Senescent cells are not dead ordying cells; they are actually resistant to programmed cell death(apoptosis), and have been maintained in their nondividing state for aslong as three years. These cells are very much alive and metabolicallyactive, but they do not divide. The nondividing state of senescent cellshas not yet been found to be reversible by any biological, chemical, orviral agent.

As used herein, the term growth medium generally refers to a mediumsufficient for the culturing of umbilical cord tissue-derived cells. Inparticular, one presently preferred medium for the culturing of thecells of the invention in comprises Dulbecco's Modified Essential Media(DMEM). Particularly preferred is DMEM-low glucose (DMEM-LG)(Invitrogen, Carlsbad, Calif.). The DMEM-LG is preferably supplementedwith serum, most preferably fetal bovine serum or human serum.Typically, 15% (v/v) fetal bovine serum (e.g. defined fetal bovineserum, Hyclone, Logan Utah) is added, along withantibiotics/antimycotics ((preferably 100 Unit/milliliter penicillin,100 milligrams/milliliter streptomycin, and 0.25 microgram/milliliteramphotericin B; Invitrogen, Carlsbad, Calif.)), and 0.001% (v/v)2-mercaptoethanol (Sigma, St. Louis Mo.). In some cases different growthmedia are used, or different supplementations are provided, and theseare normally indicated in the text as supplementations to Growth Medium.In certain chemically-defined media the cells may be grown without serumpresent at all. In such cases, the cells may require certain growthfactors, which can be added to the medium to support and sustain thecells. Presently preferred factors to be added for growth on serum-freemedia include one or more of bFGF, EGF, IGF-I, and PDGF. In morepreferred embodiments, two, three or all four of the factors are add toserum free or chemically defined media. In other embodiments, LIF isadded to serum-free medium to support or improve growth of the cells.

Also relating to the present invention, the term standard growthconditions, as used herein refers to culturing of cells at 37° C., in astandard atmosphere comprising 5% CO₂. Relative humidity is maintainedat about 100%. While the foregoing conditions are useful for culturing,it is to be understood that such conditions are capable of being variedby the skilled artisan who will appreciate the options available in theart for culturing cells.

The term effective amount refers to a concentration or amount of acompound, material, or composition, as described herein, that iseffective to achieve a particular biological result. Such resultsinclude, but are not limited to, the regeneration, repair, orimprovement of skeletal tissue, the improvement of blood flow, and/orthe stimulation and/or support of angiogenesis in peripheral ischemiapatients. Such effective activity may be achieved, for example, byadministering the cells and/or compositions of the present invention toperipheral ischemia patients. With respect to umbilical cordtissue-derived cells as administered to a patient in vivo, an effectiveamount may range from as few as several hundred or fewer to as many asseveral million or more. In specific embodiments, an effective amountmay range from 10³-10¹¹, more specifically at least about 10⁴ cells. Itwill be appreciated that the number of cells to be administered willvary depending on the specifics of the disorder to be treated, includingbut not limited to size or total volume/surface area to be treated, andproximity of the site of administration to the location of the region tobe treated, among other factors familiar to the medicinal biologist.

The terms treat, treating or treatment refer to any success or indiciaof success in the attenuation or amelioration of an injury, pathology orcondition, including any objective or subjective parameter such asabatement, remission, diminishing of symptoms or making the injury,pathology, or condition more tolerable to the patient, slowing in therate of degeneration or decline, making the final point of degenerationless debilitating, improving a subject's physical or mental well-being,or prolonging the length of survival. The treatment or amelioration ofsymptoms can be based on objective or subjective parameters; includingthe results of a physical examination, neurological examination, and/orpsychiatric evaluations.

The terms effective period (or time) and effective conditions refer to aperiod of time or other controllable conditions (e.g., temperature,humidity for in vitro methods), necessary or preferred for an agent orpharmaceutical composition to achieve its intended result.

The terms patient or subject are used interchangeably herein, and referto animals, preferably mammals, and more preferably humans, who aretreated with the pharmaceutical or therapeutic compositions or inaccordance with the methods described herein.

Ischemia refers to any decrease or stoppage in the blood supply to anybodily organ, tissue, or part caused by any constriction or obstructionof the vasculature. Ischemic episode or ischemic event are usedinterchangeably herein and refer to any transient or permanent period ofischemia. Peripheral ischemia refers to any decrease or stoppage in theblood supply to any bodily organ, tissue, or part, excluding the heart,caused by any constriction or obstruction of the vasculature. Peripheralvascular disease (PVD) refers to diseases of the blood vessels outsidethe heart and brain. It often involves a narrowing of the blood vesselscarrying blood to the extremities, and results from two types ofcirculation disorders, namely, (1) functional peripheral vasculardisease that involves short-term spasm that narrows the blood vessels;and (2) organic peripheral vascular disease that involves structuralchanges in the blood vessels, such as caused by inflammation or fattyblockages, for example. As used herein, PVD also encompasses Raynouds,intermittent claudication and critical limb ischemia.

The term pharmaceutically acceptable carrier or medium, which may beused interchangeably with the term biologically compatible carrier ormedium, refers to reagents, cells, compounds, materials, compositions,and/or dosage forms that are not only compatible with the cells andother agents to be administered therapeutically, but also are, withinthe scope of sound medical judgment, suitable for use in contact withthe tissues of human beings and animals without excessive toxicity,irritation, allergic response, or other complication commensurate with areasonable benefit/risk ratio. As described in greater detail herein,pharmaceutically acceptable carriers suitable for use in the presentinvention include liquids, semi-solid (e.g., gels) and solid materials(e.g., cell scaffolds and matrices, tubes sheets and other suchmaterials as known in the art and described in greater detail herein).These semi-solid and solid materials may be designed to resistdegradation within the body (non-biodegradable) or they may be designedto degrade within the body (biodegradable, bioerodable). A biodegradablematerial may further be bioresorbable or bioabsorbable, i.e., it may bedissolved and absorbed into bodily fluids (water-soluble implants areone example), or degraded and ultimately eliminated from the body,either by conversion into other materials or breakdown and eliminationthrough natural pathways. The biodegradation rate can vary according tothe desired release rate once implanted in the body. The matrixdesirably also acts as a temporary scaffold until replaced by newlygrown skeletal muscle, pericytes, vascular smooth muscle, or vascularendothelial tissue. Therefore, in one embodiment, the matrix providesfor sustained release of the other agents used in conjunction with theumbilical cord tissue-derived cells and may provide a structure fordeveloping tissue growth in the patient. In other embodiments, thematrix simply provides a temporary scaffold for the developing tissue.The matrix can be in particulate form (macroparticles greater than 10microns in diameter or microparticles less than 10 microns in diameter),or can be in the form of a structurally stable, three-dimensionalimplant (e.g., a scaffold). The implant can be, for example, a cube,cylinder, tube, block, film, sheet, or an appropriate anatomical form.

Several terms are used herein with respect to cell or tissuetransplantation. The terms autologous transfer, autologoustransplantation, autograft and the like refer to transplantation whereinthe transplant donor is also the transplant recipient. The termsallogeneic transfer, allogeneic transplantation, allograft and the likerefer to transplantation wherein the transplant donor is of the samespecies as the transplant recipient, but is not the recipient. A celltransplant in which the donor cells have been histocompatibly matchedwith a recipient is sometimes referred to as a syngeneic transfer. Theterms xenogeneic transfer, xenogeneic transplantation, xenograft and thelike refer to transplantation wherein the transplant donor is of adifferent species than the transplant recipient.

In its various embodiments described herein, the present inventionfeatures methods and pharmaceutical compositions for treatment ofperipheral vascular disease that utilize progenitor cells and cellpopulations derived from umblicus tissue. These methods andpharmaceutical compositions are designed to stimulate and supportangiogenesis, to improve blood flow, to regenerate, repair, and improveskeletal muscle damaged by a peripheral ischemic event, and/or toprotect skeletal muscle from ischemic damage. The cells, cellpopulations and preparations comprising cell lysates, conditioned mediaand the like, used in the pharmaceutical preparations and methods of thepresent invention are described in detail in US Patent Publication Nos.2005/0058631 and 2005/0054098, and also herein below.

One embodiment of the invention is a method of treating a peripheralvascular disease with an umbilical cord tissue-derived cell as describedin herein. In one embodiment of the invention, the cells are provided aspart of a pharmaceutical composition.

In another embodiment of the invention, the method of treating aperipheral vascular disease utilizes fibrin glue (also known as a fibrinsealant). As used herein, the term “fibrin glue” shall encompass anybiological or synthetic substance used to create a fibrin clot. In oneembodiment, the fibrin glue is scaffold for cell implantation.Optimally, the fibrin glue has the ability to withstand, for asufficient period of time, its degradation inside the body. In oneembodiment, the fibrin glue comprises fibrinogen (factor I), such ase.g. recombinant fibrinogen or fibrinogen purified from blood, andthrombin. In another embodiment, the fibrin glue comprises fibrinogen,thrombin, factor XIII and optionally one or more of calcium, aprotinin,fibronectin and plasminogen. In yet another embodiment, the fibrin gluecomprises fibrinogen, thrombin and optionally one or more of factorXIII, anti-fribinolytic agents (e.g. transexamic acid), stabilizers(e.g. arginine hydrocholoride), calcium, aprotinin, fibronectin andplasminogen. In an alternate embodiment, the fibrin glue issubstantially free of added protease inhibitors. In yet anotherembodiment, the fibrin glue comprises BAC2 (fibrinogen) and thrombin. Inan alternate embodiment, the fibrin glue is EVICEL® fibrin glue (EVICEL®Fibrin sealant (Human), Omrix Pharmaceuticals) (thrombin and BAC2(fibrinogen)). In one embodiment, the fibrin glue may be provided as amulti-component system, which is mixed prior to use, with one componentcomprising fibrin (and optionally factor XIII) and another componentcomprising thrombin (and optionally calcium). In another embodiment, thefibrin glue is a scaffold as described in U.S. Provisional ApplicationNo. 61/372,929 (filed Aug. 12, 2010), the disclosure of which isincorporated by reference in its entirety as it pertains to thedescription, characterization and use of fibrin scaffolds.

The fibrin glue may be administered simultaneously with, or before, orafter umbilical-cord tissue derived cells as described herein(umbilical-derived cells). In one embodiment, the fibrin glue andumbilical-derived cells as described herein are provided in the form ofa composition such as e.g. a pharmaceutical composition. In oneembodiment, the composition is administered locally (such as e.g. viaintramuscular injection or injection into adipose depots in muscle). Inanother embodiment, the fibrin glue and umbilical-derived cells asdescribed herein are administered locally (such as e.g. viaintramuscular injection or injection into adipose depots in muscle). Inanother embodiment, the composition, or the cells and fibrin glue, areadministered by injection into interstitial spaces so as not to directlyenter into circulation. In another embodiment, the method comprisesproviding the cells in fibrinogen to which thrombin is added immediatelyprior to local delivery. In one embodiment, the fibrin glue comprisesfrom about 16 to about 24 IU/ml, alternatively from about 18 to 22 IU/mlof thrombin and from about 39.3 to about 60.7 mg/ml, alternatively fromabout 45 to about 60 mg/ml, alternatively from about 40 to about 55mg/ml, alternatively from about 45 to about 55 mg/ml of fibrinogen (e.g.BAC2). In yet another embodiment, the fibrin glue comprises about 16,17, 18, 19, 20, 21, 22, 23 or 24 IU/ml of thrombin and about 40, 43, 45,48, 50, 52, 53, 58 or 60 mg/ml of fibrinogen. In one embodiment, about1×10⁶ cells are used with the fibrin glue.

According to the methods described herein, a mammalian umbilical cord isrecovered upon or shortly after termination of either a full-term orpre-term pregnancy, for example, after expulsion of after birth. Theumbilical cord tissue may be transported from the birth site to alaboratory in a sterile container such as a flask, beaker, culture dish,or bag. The container may have a solution or medium, including but notlimited to a salt solution, such as Dulbecco's Modified Eagle's Medium(DMEM) (also known as Dulbecco's Minimal Essential Medium) or phosphatebuffered saline (PBS), or any solution used for transportation of organsused for transplantation, such as University of Wisconsin solution orperfluorochemical solution. One or more antibiotic and/or antimycoticagents, such as but not limited to penicillin, streptomycin,amphotericin B, gentamicin, and nystatin, may be added to the medium orbuffer. The tissue may be rinsed with an anticoagulant solution such asheparin-containing solution. It is preferable to keep the tissue atabout 4-10° C. prior to extraction of umbilical cord tissue-derivedcells. It is even more preferable that the tissue not be frozen prior toextraction of umbilical cord tissue-derived cells.

Isolation of umbilical-derived cells preferably occurs in an asepticenvironment. The umbilical cord may be separated from the placenta bymeans known in the art. Blood and debris are preferably removed from thetissue prior to isolation of umbilical cord tissue-derived cells. Forexample, the umbilical tissue may be washed with buffer solution,including but not limited to phosphate buffered saline. The wash bufferalso may comprise one or more antimycotic and/or antibiotic agents,including but not limited to penicillin, streptomycin, amphotericin B,gentamicin, and nystatin.

Umbilical tissue comprising a whole umbilical cord or a fragment orsection thereof is disaggregated by mechanical force (mincing or shearforces). In a presently preferred embodiment, the isolation procedurealso utilizes an enzymatic digestion process. Many enzymes are known inthe art to be useful for the isolation of individual cells from complextissue matrices to facilitate growth in culture. Digestion enzymes rangefrom weakly digestive (e.g. deoxyribonucleases and the neutral protease,dispase) to strongly digestive (e.g. papain and trypsin), and areavailable commercially. A nonexhaustive list of enzymes compatibleherewith includes mucolytic enzyme activities, metalloproteases, neutralproteases, serine proteases (such as trypsin, chymotrypsin, orelastase), and deoxyribonucleases. Presently preferred are enzymeactivities selected from metalloproteases, neutral proteases andmucolytic activities. For example, collagenases are known to be usefulfor isolating various cells from tissues. Deoxyribonucleases can digestsingle-stranded DNA and can minimize cell-clumping during isolation.Preferred methods involve enzymatic treatment with for examplecollagenase and dispase, or collagenase, dispase, and hyaluronidase. Incertain embodiments, a mixture of collagenase and the neutral proteasedispase are used in the dissociating step. More specific embodimentsemploy digestion in the presence of at least one collagenase fromClostridium histolyticum, and either of the protease activities, dispaseand thermolysin. Still other embodiments employ digestion with bothcollagenase and dispase enzyme activities. Also utilized are methodsthat include digestion with a hyaluronidase activity in addition tocollagenase and dispase activities. The skilled artisan will appreciatethat many such enzyme treatments are known in the art for isolatingcells from various tissue sources. For example, the enzyme blends fortissue disassociation sold under the trade name LIBERASE® (Roche,Indianapolis, Ind.) are suitable for use in the instant methods. Othersources of enzymes are known, and the skilled artisan may also obtainsuch enzymes directly from their natural sources. The skilled artisan isalso well-equipped to assess new or additional enzymes or enzymecombinations for their utility in isolating the cells of the invention.Preferred enzyme treatments are 0.5, 1, 1.5, or 2 hours long or longer.In other preferred embodiments, the tissue is incubated at 37° C. duringthe enzyme treatment of the dissociation step.

In some embodiments of the invention, umbilical tissue is separated intosections comprising various aspects of the tissue, such as neonatal,neonatal/maternal, and maternal aspects of the placenta, for instance.The separated sections then are dissociated by mechanical and/orenzymatic dissociation according to the methods described herein. Cellsof neonatal or maternal lineage may be identified by any means known inthe art, for example, by karyotype analysis or in situ hybridization fora Y chromosome.

Isolated cells or umbilical tissue from which cells are derived may beused to initiate, or seed, cell cultures. Isolated cells are transferredto sterile tissue culture vessels either uncoated or coated withextracellular matrix or ligands such as laminin, collagen (native,denatured or crosslinked), gelatin, fibronectin, and other extracellularmatrix proteins. Umbilical cord tissue-derived cells are cultured in anyculture medium capable of sustaining growth of the cells such as, butnot limited to, DMEM (high or low glucose), advanced DMEM, DMEM/MCDB201, Eagle's basal medium, Ham's F10 medium (F10), Ham's F-12 medium(F12), Iscove's modified Dulbecco's medium, Mesenchymal Stem Cell GrowthMedium (MSCGM), DMEM/F12, RPMI 1640, and serum/media free medium soldunder the trade name CELL-GRO-FREE® (Mediatech, Inc., Herndon, Va.). Theculture medium may be supplemented with one or more componentsincluding, for example, fetal bovine serum (FBS), preferably about 2-15%(v/v); equine serum (ES); human serum (HS); beta-mercaptoethanol (BME or2-ME), preferably about 0.001% (v/v); one or more growth factors, forexample, platelet-derived growth factor (PDGF), epidermal growth factor(EGF), fibroblast growth factor (FGF), vascular endothelial growthfactor (VEGF), insulin-like growth factor-1 (IGF-1), leukocyteinhibitory factor (LIF) and erythropoietin (EPO); amino acids, includingL-valine; and one or more antibiotic and/or antimycotic agents tocontrol microbial contamination, such as penicillin G, streptomycinsulfate, amphotericin B, gentamicin, and nystatin, either alone or incombination. The culture medium preferably comprises Growth Medium asdefined in the Examples below.

The cells are seeded in culture vessels at a density to allow cellgrowth. In a preferred embodiment, the cells are cultured at about 0 toabout 5 percent by volume CO₂ in air. In some preferred embodiments, thecells are cultured at about 2 to about 25 percent O₂ in air, preferablyabout 5 to about 20 percent O₂ in air. The cells preferably are culturedat a temperature of about 25 to about 40° C. and more preferably arecultured at 37° C. The cells are preferably cultured in an incubator.The medium in the culture vessel can be static or agitated, for example,using a bioreactor. Umbilical cord tissue-derived cells preferably aregrown under low oxidative stress (e.g., with addition of glutathione,Vitamin C, Catalase, Vitamin E, N-Acetylcysteine). “Low oxidativestress,” as used herein, refers to conditions of no or minimal freeradical damage to the cultured cells.

Methods for the selection of the most appropriate culture medium, mediumpreparation, and cell culture techniques are well known in the art andare described in a variety of sources, including Doyle et al., (eds.),1995, CELL & TISSUE CULTURE: LABORATORY PROCEDURES, John Wiley & Sons,Chichester; and Ho and Wang (eds.), 1991, ANIMAL CELL BIOREACTORS,Butterworth-Heinemann, Boston, which are incorporated herein byreference.

After culturing the isolated cells or tissue fragments for a sufficientperiod of time, umbilical cord tissue-derived cells will have grown out,either as a result of migration from the umbilical tissue or celldivision, or both. In some embodiments of the invention, umbilical cordtissue-derived cells are passaged, or removed to a separate culturevessel containing fresh medium of the same or a different type as thatused initially, where the population of cells can be mitoticallyexpanded. The cells of the invention may be used at any point betweenpassage 0 and senescence. The cells preferably are passaged betweenabout 3 and about 25 times, more preferably are passaged about 4 toabout 12 times, and preferably are passaged 10 or 11 times. Cloningand/or subcloning may be performed to confirm that a clonal populationof cells has been isolated.

In some aspects of the invention, the different cell types present inumbilical tissue are fractionated into subpopulations from which theumbilical cord tissue-derived cells can be isolated. Fractionation orselection may be accomplished using standard techniques for cellseparation including, but not limited to, enzymatic treatment todissociate umbilical tissue into its component cells, followed bycloning and selection of specific cell types, including but not limitedto selection based on morphological and/or biochemical markers;selective growth of desired cells (positive selection), selectivedestruction of unwanted cells (negative selection); separation basedupon differential cell agglutinability in the mixed population as, forexample, with soybean agglutinin; freeze-thaw procedures; differentialadherence properties of the cells in the mixed population; filtration;conventional and zonal centrifugation; centrifugal elutriation(counter-streaming centrifugation); unit gravity separation;countercurrent distribution; electrophoresis; and fluorescence activatedcell sorting (FACS). For a review of clonal selection and cellseparation techniques, see Freshney, 1994, CULTURE OF ANIMAL CELLS: AMANUAL OF BASIC TECHNIQUES, 3rd Ed., Wiley-Liss, Inc., New York, whichis incorporated herein by reference.

The culture medium is changed as necessary, for example, by carefullyaspirating the medium from the dish, for example, with a pipette, andreplenishing with fresh medium. Incubation is continued until asufficient number or density of cells accumulates in the dish. Theoriginal explanted tissue sections may be removed and the remainingcells trypsinized using standard techniques or using a cell scraper.After trypsinization, the cells are collected, removed to fresh mediumand incubated as above. In some embodiments, the medium is changed atleast once at approximately 24 hours post-trypsinization to remove anyfloating cells. The cells remaining in culture are considered to beumbilical cord tissue-derived cells.

Umbilical cord tissue-derived cells may be cryopreserved. Accordingly,in a preferred embodiment described in greater detail below, umbilicalcord tissue-derived cells for autologous transfer (for either the motheror child) may be derived from appropriate umbilical tissues followingthe birth of a child, then cryopreserved so as to be available in theevent they are later needed for transplantation.

Umbilical cord tissue-derived cells may be characterized, for example,by growth characteristics (e.g., population doubling capability,doubling time, passages to senescence), karyotype analysis (e.g., normalkaryotype; maternal or neonatal lineage), flow cytometry (e.g., FACSanalysis), immunohistochemistry and/or immunocytochemistry (e.g., fordetection of epitopes), gene expression profiling (e.g., gene chiparrays; polymerase chain reaction (for example, reverse transcriptasePCR, real time PCR, and conventional PCR)), protein arrays, proteinsecretion (e.g., by plasma clotting assay or analysis of PDC-conditionedmedium, for example, by Enzyme Linked ImmunoSorbent Assay (ELISA)),mixed lymphocyte reaction (e.g., as measure of stimulation of PBMCs),and/or other methods known in the art.

Examples of cells derived from umbilicus tissue were deposited with theAmerican Type Culture Collection (ATCC, 10801 University Blvd.,Manassas, Va.) on Jun. 10, 2004, and assigned ATCC Accession Numbers asfollows: (1) strain designation UMB 022803 (P7) was assigned AccessionNo. PTA-6067; and (2) strain designation UMB 022803 (P17) was assignedAccession No. PTA-6068.

In various embodiments, the umbilical cord tissue-derived cells possessone or more of the following growth features (1) they require L-valinefor growth in culture; (2) they are capable of growth in atmospherescontaining oxygen from about 5% to at least about 20% (3) they have thepotential for at least about 40 doublings in culture before reachingsenescence; and (4) they attach and expand on a coated or uncoatedtissue culture vessel, wherein the coated tissue culture vesselcomprises a coating of gelatin, laminin, collagen, polyornithine,vitronectin or fibronectin.

In certain embodiments the umbilical cord tissue-derived cells possess anormal karyotype, which is maintained as the cells are passaged.Karyotyping is particularly useful for identifying and distinguishingneonatal from maternal cells derived from placenta. Methods forkaryotyping are available and known to those of skill in the art.

In other embodiments, the umbilical cord tissue-derived cells may becharacterized by production of certain proteins, including (1)production of at least one of tissue factor, vimentin, and alpha-smoothmuscle actin; and (2) production of at least one of CD10, CD13, CD44,CD73, CD90, PDGFr-alpha, PD-L2 and HLA-A,B,C cell surface markers, asdetected by flow cytometry. In other embodiments, the umbilical cordtissue-derived cells may be characterized by lack of production of atleast one of CD31, CD34, CD45, CD80, CD86, CD117, CD141, CD178, B7-H2,HLA-G, and HLA-DR,DP,DQ cell surface markers, as detected by flowcytometry. Particularly preferred are cells that produce at least two oftissue factor, vimentin, and alpha-smooth muscle actin. More preferredare those cells producing all three of the proteins tissue factor,vimentin, and alpha-smooth muscle actin.

In other embodiments, the umbilical cord tissue-derived cells may becharacterized by gene expression, which relative to a human cell that isa fibroblast, a mesenchymal stem cell, or an iliac crest bone marrowcell, is increased for a gene encoding at least one of interleukin 8;reticulon 1; chemokine (C-X-C motif) ligand 1 (melonoma growthstimulating activity, alpha); chemokine (C-X-C motif) ligand 6(granulocyte chemotactic protein 2); chemokine (C-X-C motif) ligand 3;and tumor necrosis factor, alpha-induced protein 3.

In yet other embodiments, the umbilical cord tissue-derived cells may becharacterized by gene expression, which relative to a human cell that isa fibroblast, a mesenchymal stem cell, or an iliac crest bone marrowcell, is reduced for a gene encoding at least one of: short staturehomeobox 2; heat shock 27 kDa protein 2; chemokine (C-X-C motif) ligand12 (stromal cell-derived factor 1); elastin (supravalvular aorticstenosis, Williams-Beuren syndrome); Homo sapiens mRNA; cDNADKFZp586M2022 (from clone DKFZp586M2022); mesenchyme homeo box 2 (growtharrest-specific homeo box); sine oculis homeobox homolog 1 (Drosophila);crystallin, alpha B; disheveled associated activator of morphogenesis 2;DKFZP586B2420 protein; similar to neuralin 1; tetranectin (plasminogenbinding protein); src homology three (SH3) and cysteine rich domain;cholesterol 25-hydroxylase; runt-related transcription factor 3;interleukin 11 receptor, alpha; procollagen C-endopeptidase enhancer;frizzled homolog 7 (Drosophila); hypothetical gene BC008967; collagen,type VIII, alpha 1; tenascin C (hexabrachion); iroquois homeobox protein5; hephaestin; integrin, beta 8; synaptic vesicle glycoprotein 2;neuroblastoma, suppression of tumorigenicity 1; insulin-like growthfactor binding protein 2, 36 kDa; Homo sapiens cDNA FLJ12280 fis, cloneMAMMA1001744; cytokine receptor-like factor 1; potassiumintermediate/small conductance calcium-activated channel, subfamily N,member 4; integrin, beta 7; transcriptional co-activator withPDZ-binding motif (TAZ); sine oculis homeobox homolog 2 (Drosophila);KIAA1034 protein; vesicle-associated membrane protein 5 (myobrevin);EGF-containing fibulin-like extracellular matrix protein 1; early growthresponse 3; distal-less homeo box 5; hypothetical protein FLJ20373;aldo-keto reductase family 1, member C3 (3-alpha hydroxysteroiddehydrogenase, type II); biglycan; transcriptional co-activator withPDZ-binding motif (TAZ); fibronectin 1; proenkephalin; integrin,beta-like 1 (with EGF-like repeat domains); Homo sapiens mRNA fulllength insert cDNA clone EUROIMAGE 1968422; EphA3; KIAA0367 protein;natriuretic peptide receptor C/guanylate cyclase C (atrionatriureticpeptide receptor C); hypothetical protein FLJ14054; Homo sapiens mRNA;cDNA DKFZp564B222 (from clone DKFZp564B222); BCL2/adenovirus E1B 19 kDainteracting protein 3-like; AE binding protein 1; and cytochrome coxidase subunit VIIa polypeptide 1 (muscle).

In other embodiments, the umbilical cord tissue-derived cells may becharacterized by secretion of at least one of MCP-1, IL-6, IL-8, GCP-2,HGF, KGF, FGF, HB-EGF, BDNF, TPO, MIP1b, RANTES, and TIMP1. In someembodiments, the umbilical cord tissue-derived cells may becharacterized by lack of secretion of at least one of TGF-beta2, ANG2,PDGFbb, MIP1a and VEGF, as detected by ELISA.

In some preferred embodiments, the cells are derived from umbilical cordtissue substantially free of blood, are capable of self-renewal andexpansion in culture, require L-valine for growth, can grow in at leastabout 5% oxygen, and comprise at least one of the followingcharacteristics: potential for at least about 40 doublings in culture;attachment and expansion on a coated or uncoated tissue culture vesselthat comprises a coating of gelatin, laminin, collagen, polyornithine,vitronectin, or fibronectin; production of vimentin and alpha-smoothmuscle actin; production of CD10, CD13, CD44, CD73, and CD90; and,expression of a gene, which relative to a human cell that is afibroblast, a mesenchymal stem cell, or an iliac crest bone marrow cell,is increased for a gene encoding interleukin 8 and reticulon 1. In someembodiments, such cells do not produce CD45 and CD117. The cells asdescribed in this paragraph can be used in methods for treating apatient having peripheral vascular disease, can be used inpharmaceutical compositions for treating peripheral vascular disease,for example, wherein such compositions comprise the cells having thesecharacteristics and a pharmaceutically acceptable carrier, and can beused in kits for making, using, and practicing such methods andpharmaceutical compositions as described and exemplified herein. Inaddition, the cells as described in this paragraph can be used togenerate conditioned cell culture media or to make preparations such ascell extracts and subcellular fractions that can be used for making,using, and practicing such methods and pharmaceutical compositions asdescribed and exemplified herein.

In preferred embodiments, the cells do not express telomerase (hTert).Accordingly, one embodiment of the invention is umbilical-derived cellsthat do not express telomerase (hTert) and that have one or more of thecharacteristics disclosed herein.

In one embodiment of the invention, the cells are isolated from humanumbilical cord tissue substantially free of blood, capable ofself-renewal and expansion in culture and lack the production of CD117and/or telomerase. The cells optionally (i) express oxidized low densitylipoprotein receptor 1, reticulon, chemokine receptor ligand 3, and/orgranulocyte chemotactic protein; and/or (ii) do not express CD31, CD34or CD45; and/or (iii) express, relative to a human fibroblast,mesenchymal stem cell, or iliac crest bone marrow cell, increased levelsof interleukin 8 or reticulon 1; and/or (iv) have the potential todifferentiate into cells of at least a skeletal muscle, vascular smoothmuscle, pericyte or vascular endothelium phenotype; and/or (v) expressCD10, CD13, CD44, CD73, and CD90.

In another embodiment of the invention, the cells are isolated fromhuman umbilical cord tissue substantially free of blood, capable ofself-renewal and expansion in culture and lack the production of CD117,CD34, CD31 and/or telomerase. In yet another embodiment of theinvention, the cells are isolated from human umbilical cord tissuesubstantially free of blood, capable of self-renewal and expansion inculture and lack the production of CD117, CD45, CD34, CD31 and/ortelomerase.

Among cells that are presently preferred for use with the invention inseveral of its aspects are umbilical cord tissue-derived cells havingthe characteristics described above and more particularly those whereinthe cells have normal karyotypes and maintain normal karyotypes withpassaging, and further wherein the cells express each of the markersCD10, CD13, CD44, CD73, CD90, PDGFr-alpha, and HLA-A,B,C, wherein thecells produce the immunologically-detectable proteins which correspondto the listed markers. Still more preferred are those cells which inaddition to the foregoing do not produce proteins corresponding to anyof the markers CD31, CD34, CD45, CD117, CD141, or HLA-DR,DP,DQ, asdetected by flow cytometry.

Certain cells having the potential to differentiate along lines leadingto various phenotypes are unstable and thus can spontaneouslydifferentiate. Presently preferred for use with the invention are cellsthat do not spontaneously differentiate, for example along myoblast,skeletal muscle, vascular smooth muscle, pericyte, hemangiogenic,angiogenic, vasculogenic, or vascular endothelial lines. Preferredcells, when grown in Growth Medium, are substantially stable withrespect to the cell markers produced on their surface, and with respectto the expression pattern of various genes, for example as determinedusing a medical diagnostic test sold under the trade name GENECHIP(Affymetrix, Inc., Santa Clara, Calif.). The cells remain substantiallyconstant, for example in their surface marker characteristics overpassaging, through multiple population doublings.

Another aspect of the invention features use of populations of theumbilical cord tissue-derived cells described above. In someembodiments, the cell population is heterogeneous. A heterogeneous cellpopulation of the invention may comprise at least about 5%, 10%, 20%,30%, 40%, 50%, 60%, 70%, 80%, 90%, or 95% umbilical cord tissue-derivedcells of the invention. The heterogeneous cell populations of theinvention may further comprise stem cells or other progenitor cells,such as myoblasts or other muscle progenitor cells, hemangioblasts, orblood vessel precursor cells, or it may further comprise fullydifferentiated skeletal muscle cells, smooth muscle cells, pericytes, orblood vessel endothelial cells. In some embodiments, the population issubstantially homogeneous, i.e., comprises substantially only umbilicalcord tissue-derived cells (preferably at least about 96%, 97%, 98%, 99%or more umbilical cord tissue-derived cells). The homogeneous cellpopulation of the invention may comprise umbilicus- or placenta-derivedcells. Homogeneous populations of umbilicus-derived cells are preferablyfree of cells of maternal lineage. Homogeneous populations ofplacenta-derived cells may be of neonatal or maternal lineage.Homogeneity of a cell population may be achieved by any method known inthe art, for example, by cell sorting (e.g., flow cytometry) or byclonal expansion in accordance with known methods. Thus, preferredhomogeneous cell populations may comprise a clonal cell line ofumbilical cord tissue-derived cells. Such populations are particularlyuseful when a cell clone with highly desirable functionality has beenisolated.

Also provided herein is the use of populations of cells incubated in thepresence of one or more factors, or under conditions, that stimulatestem cell differentiation along a vascular smooth muscle, vascularendothelial, pericyte, or skeletal muscle pathway. Such factors areknown in the art and the skilled artisan will appreciate thatdetermination of suitable conditions for differentiation can beaccomplished with routine experimentation. Optimization of suchconditions can be accomplished by statistical experimental design andanalysis, for example response surface methodology allows simultaneousoptimization of multiple variables, for example in a biological culture.Presently preferred factors include, but are not limited to growth ortrophic factors, chemokines, cytokines, cellular products, demethylatingagents, and other stimuli which are now known or later determined tostimulate differentiation, for example, of stem cells along angiogenic,hemangiogenic, vasculogenic, skeletal muscle, vascular smooth muscle,pericyte, or vascular endothelial pathways or lineages.

Umbilical cord tissue-derived cells may also be genetically modified toproduce therapeutically useful gene products, to produce angiogenicagents to facilitate or support additional blood vessel formation orgrowth, or to produce factors to recruit endothelial progenitor cells tothe area of ischemic damage. Endothelial progenitor cells facilitatevasculogenesis and blood flow, particularly following an ischemic event(Urbich C and Dimmeler S (2004) Circ. Res. 95:343-53). Factors that playa role in endothelial cell recruitment include, but are not limited toVEGF, stromal derived factor-1 (SDF-1), erythropoietin (EPO), G-CSF,statins, strogen, PPARγ, CXCR4, FGF, and HGF. Genetic modification maybe accomplished using any of a variety of vectors including, but notlimited to, integrating viral vectors, e.g., retrovirus vector oradeno-associated viral vectors; non-integrating replicating vectors,e.g., papilloma virus vectors, SV40 vectors, adenoviral vectors; orreplication-defective viral vectors. Other methods of introducing DNAinto cells include the use of liposomes, electroporation, a particlegun, or by direct DNA injection.

Hosts cells are preferably transformed or transfected with DNAcontrolled by or in operative association with, one or more appropriateexpression control elements such as promoter or enhancer sequences,transcription terminators, polyadenylation sites, among others, and aselectable marker. Any promoter may be used to drive the expression ofthe inserted gene. For example, viral promoters include, but are notlimited to, the CMV promoter/enhancer, SV40, papillomavirus,Epstein-Barr virus or elastin gene promoter. In some embodiments, thecontrol elements used to control expression of the gene of interest canallow for the regulated expression of the gene so that the product issynthesized only when needed in vivo. If transient expression isdesired, constitutive promoters are preferably used in a non-integratingand/or replication-defective vector. Alternatively, inducible promoterscould be used to drive the expression of the inserted gene whennecessary. Inducible promoters include, but are not limited to, thoseassociated with metallothionein and heat shock proteins.

Following the introduction of the foreign DNA, engineered cells may beallowed to grow in enriched media and then switched to selective media.The selectable marker in the foreign DNA confers resistance to theselection and allows cells to stably integrate the foreign DNA as, forexample, on a plasmid, into their chromosomes and grow to form fociwhich, in turn, can be cloned and expanded into cell lines. This methodcan be advantageously used to engineer cell lines that express the geneproduct.

The cells of the invention may be genetically engineered to “knock out”or “knock down” expression of factors that promote inflammation orrejection at the implant site. Negative modulatory techniques for thereduction of target gene expression levels or target gene productactivity levels are discussed below. “Negative modulation,” as usedherein, refers to a reduction in the level and/or activity of targetgene product relative to the level and/or activity of the target geneproduct in the absence of the modulatory treatment. The expression of agene native to a skeletal muscle cell, vascular smooth muscle cell,pericyte, vascular endothelial cell, or progenitor cells thereof can bereduced or knocked out using a number of techniques including, forexample, inhibition of expression by inactivating the gene using thehomologous recombination technique. Typically, an exon encoding animportant region of the protein (or an exon 5′ to that region) isinterrupted by a positive selectable marker, e.g., neo, preventing theproduction of normal mRNA from the target gene and resulting ininactivation of the gene. A gene may also be inactivated by creating adeletion in part of a gene, or by deleting the entire gene. By using aconstruct with two regions of homology to the target gene that are farapart in the genome, the sequences intervening the two regions can bedeleted (Mombaerts et al., 1991, Proc. Nat. Acad. Sci. U.S.A.88:3084-3087). Antisense, DNAzymes, ribozymes, small interfering RNA(siRNA) and other such molecules that inhibit expression of the targetgene can also be used to reduce the level of target gene activity. Forexample, antisense RNA molecules that inhibit the expression of majorhistocompatibility gene complexes (HLA) have been shown to be mostversatile with respect to immune responses. Still further, triple helixmolecules can be utilized in reducing the level of target gene activity.These techniques are described in detail by L. G. Davis et al. (eds),1994, BASIC METHODS IN MOLECULAR BIOLOGY, 2nd ed., Appleton & Lange,Norwalk, Conn.

In other aspects, the invention utilizes cell lysates and cell solublefractions prepared from umbilical cord tissue-derived cells, orheterogeneous or homogeneous cell populations comprising umbilical cordtissue-derived cells, as well as umbilical cord tissue-derived cells orpopulations thereof that have been genetically modified or that havebeen stimulated to differentiate along a skeletal muscle, vascularsmooth muscle, pericyte, or vascular endothelium pathway. Such lysatesand fractions thereof have many utilities. Use of the cell lysatesoluble fraction (i.e., substantially free of membranes) in vivo, forexample, allows the beneficial intracellular milieu to be usedallogeneically in a patient without introducing an appreciable amount ofthe cell surface proteins most likely to trigger rejection, or otheradverse immunological responses. Methods of lysing cells are well-knownin the art and include various means of mechanical disruption, enzymaticdisruption, or chemical disruption, or combinations thereof. Such celllysates may be prepared from cells directly in their Growth Medium andthus containing secreted growth factors and the like, or may be preparedfrom cells washed free of medium in, for example, PBS or other solution.Washed cells may be resuspended at concentrations greater than theoriginal population density if preferred.

In one embodiment, whole cell lysates are prepared, e.g., by disruptingcells without subsequent separation of cell fractions. In anotherembodiment, a cell membrane fraction is separated from a solublefraction of the cells by routine methods known in the art, e.g.,centrifugation, filtration, or similar methods.

Cell lysates or cell soluble fractions prepared from populations ofumbilical cord tissue-derived cells may be used as is, furtherconcentrated, by for example, ultrafiltration or lyophilization, or evendried, partially purified, combined with pharmaceutically-acceptablecarriers or diluents as are known in the art, or combined with othercompounds such as biologicals, for example pharmaceutically usefulprotein compositions. Cell lysates or fractions thereof may be used invitro or in vivo, alone or for example, with autologous or syngeneiclive cells. The lysates, if introduced in vivo, may be introducedlocally at a site of treatment, or remotely to provide, for exampleneeded cellular growth factors to a patient.

In a further embodiment, umbilical cord tissue-derived cells can becultured in vitro to produce biological products in high yield.Umbilical cord tissue-derived cells that either naturally produce aparticular biological product of interest (e.g., a trophic factor), orthat have been genetically engineered to produce a biological product,can be clonally expanded using the culture techniques described herein.Alternatively, cells may be expanded in a medium that inducesdifferentiation to a skeletal muscle, vascular smooth muscle, pericyte,or vascular endothelial lineage. In each case, biological productsproduced by the cell and secreted into the medium can be readilyisolated from the conditioned medium using standard separationtechniques, e.g., such as differential protein precipitation,ion-exchange chromatography, gel filtration chromatography,electrophoresis, and HPLC, to name a few. A “bioreactor” may be used totake advantage of the flow method for feeding, for example, athree-dimensional culture in vitro. Essentially, as fresh media ispassed through the three-dimensional culture, the biological product iswashed out of the culture and may then be isolated from the outflow, asabove.

Alternatively, a biological product of interest may remain within thecell and, thus, its collection may require that the cells be lysed, asdescribed above. The biological product may then be purified using anyone or more of the above-listed techniques.

In other embodiments, the invention utilizes conditioned medium fromcultured umbilical cord tissue-derived cells for use in vitro and invivo as described below. Use of the cell conditioned medium allows thebeneficial trophic factors secreted by the umbilical cord tissue-derivedcells to be used allogeneically in a patient without introducing intactcells that could trigger rejection, or other adverse immunologicalresponses. Conditioned medium is prepared by culturing cells in aculture medium, then removing the cells from the medium.

Conditioned medium prepared from populations of umbilical cordtissue-derived cells may be used as is, further concentrated, forexample, by ultrafiltration or lyophilization, or even dried, partiallypurified, combined with pharmaceutically-acceptable carriers or diluentsas are known in the art, or combined with other compounds such asbiologicals, for example pharmaceutically useful protein compositions.Conditioned medium may be used in vitro or in vivo, alone or combinedwith autologous or syngeneic live cells, for example. The conditionedmedium, if introduced in vivo, may be introduced locally at a site oftreatment, or remotely to provide needed cellular growth or trophicfactors to a patient.

In another embodiment, an extracellular matrix (ECM) produced byculturing umbilical cord tissue-derived cells on liquid, solid orsemi-solid substrates is prepared, collected and utilized as analternative to implanting live cells into a subject in need of tissuerepair or replacement. Umbilical cord tissue-derived cells are culturedin vitro, on a three dimensional framework as described elsewhereherein, under conditions such that a desired amount of ECM is secretedonto the framework. The cells comprising the new tissue are removed, andthe ECM processed for further use, for example, as an injectablepreparation. To accomplish this, cells on the framework are killed andany cellular debris removed from the framework. This process may becarried out in a number of different ways. For example, the livingtissue can be flash-frozen in liquid nitrogen without acryopreservative, or the tissue can be immersed in sterile distilledwater so that the cells burst in response to osmotic pressure.

Once the cells have been killed, the cellular membranes may be disruptedand cellular debris removed by treatment with a mild detergent rinse,such as Ethylenediaminetetraacetic acid (EDTA),3-[(3-cholamidopropyl)dimethylammonio]-1-propanesulfonate (CHAPS) or azwitterionic detergent. Alternatively, the tissue can be enzymaticallydigested and/or extracted with reagents that break down cellularmembranes and allow removal of cell contents. Examples of such enzymesinclude, but are not limited to, hyaluronidase, dispase, proteases, andnucleases. Examples of detergents include non-ionic detergents such as,for example, alkylaryl polyether alcohol (TRITON X-100), octylphenoxypolyethoxy-ethanol (Rohm and Haas, Philadelphia, Pa.), BRIJ-35, apolyethoxyethanol lauryl ether (Atlas Chemical Co., San Diego, Calif.),polysorbate 20 (TWEEN 20), a polyethoxyethanol sorbitan monolaureate(Rohm and Haas, Philadelphia, Pa.), polyethylene lauryl ether (Rohm andHaas, Philadelphia, Pa.); and ionic detergents such as sodium dodecylsulfate, sulfated higher aliphatic alcohols, sulfonated alkanes andsulfonated alkylarenes containing 7 to 22 carbon atoms in a branched orunbranched chain.

The collection of the ECM can be accomplished in a variety of ways,depending at least in part on whether the new tissue has been formed ona three-dimensional framework that is biodegradable ornon-biodegradable, as in the case of metals. For example, if theframework is non-biodegradable, the ECM can be removed by subjecting theframework to sonication, high pressure water jets, mechanical scraping,or mild treatment with detergents or enzymes, or any combination of theabove.

If the framework is biodegradable, the ECM can be collected, forexample, by allowing the framework to degrade or dissolve in solution.Alternatively, if the biodegradable framework is composed of a materialthat can itself be injected along with the ECM, the framework and theECM can be processed in toto for subsequent injection. Alternatively,the ECM can be removed from the biodegradable framework by any of themethods described above for collection of ECM from a non-biodegradableframework. All collection processes are preferably designed so as not todenature the ECM.

After it has been collected, the ECM may be processed further. Forexample, the ECM can be homogenized to fine particles using techniqueswell known in the art such as by sonication, so that it can pass througha surgical needle. The components of the ECM can also be crosslinked, ifdesired, by gamma irradiation. Preferably, the ECM can be irradiatedbetween 0.25 to 2 mega rads to sterilize and crosslink the ECM. Chemicalcrosslinking using agents that are toxic, such as glutaraldehyde, ispossible but not generally preferred.

The amounts and/or ratios of proteins, such as the various types ofcollagen present in the ECM, may be adjusted by mixing the ECM producedby the cells of the invention with ECM of one or more other cell types.In addition, biologically active substances such as proteins, growthfactors and/or drugs, can be incorporated into the ECM. Exemplarybiologically active substances include tissue growth factors, such asTGF-beta, and the like, which promote healing and tissue repair at thesite of the injection. Such additional agents may be utilized in any ofthe embodiments described herein above, e.g., with whole cell lysates,soluble cell fractions, or further purified components and productsproduced by the umbilical cord tissue-derived cells.

In another aspect, the invention provides pharmaceutical compositionsthat utilize the umbilical cord tissue-derived cells, umbilical cordtissue-derived cell populations, components and products of umbilicalcord tissue-derived cells in various methods for the treatment of injuryor damage caused by a peripheral ischemic episode. Certain embodimentsencompass pharmaceutical compositions comprising live cells (umbilicalcord tissue-derived cells alone or admixed with other cell types). Otherembodiments encompass pharmaceutical compositions comprising umbilicalcord tissue-derived cell cellular components (e.g., cell lysates,soluble cell fractions, conditioned medium, ECM, or components of any ofthe foregoing) or products (e.g., trophic and other biological factorsproduced naturally by umbilical cord tissue-derived cells or throughgenetic modification, conditioned medium from umbilical cordtissue-derived cell culture). In either case, the pharmaceuticalcomposition may further comprise other active agents, such asanti-inflammatory agents, anti-apoptotic agents, antioxidants, growthfactors, myotrophic factors or myoregenerative or myoprotective drugs asknown in the art.

Examples of other components that may be added to the pharmaceuticalcompositions include, but are not limited to: (1) other myobeneficial ormyoprotective drugs, or angiobeneficial or angioprotective drugs; (2)selected extracellular matrix components, such as one or more types ofcollagen known in the art, and/or growth factors, platelet-rich plasma,and drugs (alternatively, umbilical cord tissue-derived cells may begenetically engineered to express and produce growth factors); (3)anti-apoptotic agents (e.g., erythropoietin (EPO), EPO mimetibody,thrombopoietin, insulin-like growth factor (IGF)-I, IGF-II, hepatocytegrowth factor, caspase inhibitors); (4) anti-inflammatory compounds(e.g., p38 MAP kinase inhibitors, TGF-beta inhibitors, statins, IL-6 andIL-1 inhibitors, Pemirolast, Tranilast, REMICADE® (Centocor, Inc.,Malvern, Pa.), Sirolimus, and non-steroidal anti-inflammatory drugs(NSAIDS) (such as Tepoxalin, Tolmetin, and Suprafen); (5)immunosuppressive or immunomodulatory agents, such as calcineurininhibitors, mTOR inhibitors, antiproliferatives, corticosteroids andvarious antibodies; (6) antioxidants such as probucol, vitamins C and E,coenzyme Q-10, glutathione, L-cysteine and N-acetylcysteine; (6) localanesthetics; (7) trophic factors such as Agrin, VEGF, VEGF-B, VEGF-C,VEGF-D, NEGF-1, NEGF-2, PDGF, GDF, IGF1, IGF2, EGF, and FGF; and, (8)factors that function in the recruitment and incorporation ofendothelial progenitor cells into ischemic tissue, such as VEGF, SDF-1,EPO, G-CSF, statins, estrogen, PPARγ, and CXCR4, to name only a few.

Pharmaceutical compositions of the invention comprise umbilical cordtissue-derived cells, components or products thereof, includingpreparations made from umbilical cord tissue-derived cells, formulatedwith a pharmaceutically acceptable carrier or medium. Suitablepharmaceutically acceptable carriers include water, salt solution (suchas Ringer's solution), alcohols, oils, gelatins, polyvinyl pyrrolidine,carbohydrates (such as lactose, amylose, or starch, fatty acid esters),and hydroxymethylcellulose. Such preparations can be sterilized, and ifdesired, mixed with auxiliary agents such as lubricants, preservatives,stabilizers, wetting agents, emulsifiers, salts for influencing osmoticpressure, buffers, and coloring agents. Pharmaceutical carriers suitablefor use in the present invention are known in the art and are described,for example, in Pharmaceutical Sciences (17^(th) Ed., Mack Pub. Co.,Easton, Pa.) and WO 96/05309.

Typically, but not exclusively, pharmaceutical compositions comprisingumbilical cord tissue-derived cell components or products, but not livecells, are formulated as liquids (or as solid tablets, capsules and thelike, when oral delivery is appropriate). These may be formulated foradministration by any acceptable route known in the art to achievedelivery of drugs and biological molecules to the target skeletalmuscle, vascular smooth muscle, pericyte, or vascular endothelialtissue, including, but not limited to, oral, nasal, ophthalmic andparenteral, including intravenous. Particular routes of parenteraladministration include, but are not limited to, intramuscular,subcutaneous, intraperitoneal, intrathecal, intracisternal, or viasyringes with needles or catheters with or without pump devices.

Pharmaceutical compositions comprising live umbilical cordtissue-derived cells are typically formulated as liquids, semisolids(e.g., gels (including fibrin glue)) or solids (e.g., matrices,scaffolds and the like, as appropriate for vascular or skeletal muscletissue engineering). Liquid compositions are formulated foradministration by any acceptable route known in the art to achievedelivery of live cells to the target vascular or skeletal muscletissues. Typically, these include injection or infusion, either in adiffuse fashion, or targeted to the site of peripheral ischemic injury,damage, or distress, by a route of administration including, but notlimited to, intramuscular, intravenous, or intra-arterial delivery viasyringes with needles and/or catheters with or without pump devices.

Pharmaceutical compositions comprising live cells in a semi-solid orsolid carrier are typically formulated for surgical implantation at thesite of ischemic injury, damage, or distress. It will be appreciatedthat liquid compositions also may be administered by surgicalprocedures. In particular embodiments, semi-solid or solidpharmaceutical compositions may comprise semi-permeable gels, lattices,cellular scaffolds and the like, which may be non-biodegradable orbiodegradable. For example, in certain embodiments, it may be desirableor appropriate to sequester the exogenous cells from their surroundings,yet enable the cells to secrete and deliver biological molecules (e.g.myotrophic factors, angiotrophic factors, or endothelial progenitor cellrecruitment factors) to surrounding skeletal muscle or vascular cells.In these embodiments, cells may be formulated as autonomous implantscomprising living umbilical cord tissue-derived cells or cell populationcomprising umbilical cord tissue-derived cells surrounded by anon-degradable, selectively permeable barrier that physically separatesthe transplanted cells from host tissue. Such implants are sometimesreferred to as “immunoprotective,” as they have the capacity to preventimmune cells and macromolecules from killing the transplanted cells inthe absence of pharmacologically induced immunosuppression (for a reviewof such devices and methods, see, e.g., P. A. Tresco et al., (2000) Adv.Drug Delivery Rev. 42:3-27).

In other embodiments, different varieties of degradable gels andnetworks are utilized for the pharmaceutical compositions of theinvention. For example, degradable materials particularly suitable forsustained release formulations include biocompatible polymers, such aspoly(lactic acid), poly (lactic acid-co-glycolic acid), methylcellulose,hyaluronic acid, collagen, and the like. The structure, selection anduse of degradable polymers in drug delivery vehicles have been reviewedin several publications, including, A. Domb et al., 1992, Polymers forAdvanced Technologies 3:279-292.

In other embodiments, it may be desirable or appropriate to deliver thecells on or in a biodegradable, preferably bioresorbable orbioabsorbable, scaffold or matrix. These typically three-dimensionalbiomaterials contain the living cells attached to the scaffold,dispersed within the scaffold, or incorporated in an extracellularmatrix entrapped in the scaffold. Once implanted into the target regionof the body, these implants become integrated with the host tissue,wherein the transplanted cells gradually become established (see, e.g.,Tresco, Pa., et al. (2000) supra; see also Hutmacher, D W (2001) J.Biomater. Sci. Polymer Edn. 12:107-174).

The biocompatible matrix may be comprised of natural, modified naturalor synthetic biodegradable polymers, including homopolymers, copolymersand block polymers, as well as combinations thereof. It is noted that apolymer is generally named based on the monomer from which it issynthesized.

Examples of suitable biodegradable polymers or polymer classes includefibrin, collagen, elastin, gelatin, vitronectin, fibronectin, laminin,thrombin, poly(aminoacid), oxidized cellulose, tropoelastin, silk,ribonucleic acids, deoxyribonucleic acids; proteins, polynucleotides,reconstituted basement membrane matrices, starches, dextrans, alginates,hyaluron, chitin, chitosan, agarose, polysaccharides, hyaluronic acid,poly(lactic acid), poly(glycolic acid), polyethylene glycol,decellularized tissue, self-assembling peptides, polypeptides,glycosaminoglycans, their derivatives and mixtures thereof. For bothglycolic acid and lactic acid, an intermediate cyclic dimer is typicallyprepared and purified prior to polymerization. These intermediate dimersare called glycolide and lactide, respectively. Other usefulbiodegradable polymers or polymer classes include, without limitation,aliphatic polyesters, poly(alkylene oxalates), tyrosine derivedpolycarbonates, polyiminocarbonates, polyorthoesters, polyoxaesters,polyamidoesters, polyoxaesters containing amine groups, poly(propylenefumarate), polydioxanones, polycarbonates, polyoxalates,poly(alpha-hydroxyacids), poly(esters), polyurethane, poly(esterurethane), poly(ether urethane), polyanhydrides, polyacetates,polycaprolactones, poly(orthoesters), polyamino acids, polyamides andblends and copolymers thereof. Additional useful biodegradable polymersinclude, without limitation stereopolymers of L- and D-lactic acid,copolymers of bis(para-carboxyphenoxy) propane and sebacic acid, sebacicacid copolymers, copolymers of caprolactone, poly(lacticacid)/poly(glycolic acid)/polyethyleneglycol copolymers, copolymers ofpolyurethane and poly(lactic acid), copolymers of alpha-amino acids,copolymers of alpha-amino acids and caproic acid, copolymers ofalpha-benzyl glutamate and polyethylene glycol, copolymers of succinateand poly(glycols), polyphosphazene, poly(hydroxyalkanoates) and mixturesthereof. Binary and ternary systems also are contemplated.

In general, a suitable biodegradable polymer for use as the matrix isdesirably configured so that it has mechanical properties that aresuitable for the intended application, remains sufficiently intact untiltissue has in-grown and healed, does not invoke an inflammatory or toxicresponse, is metabolized in the body after fulfilling its purpose, iseasily processed into the desired final product to be formed,demonstrates acceptable shelf-life, and is easily sterilized.

In one aspect of the invention, the biocompatible polymer used to formthe matrix is in the form of a hydrogel. In one embodiment of theinvention, the hydrogel comprisese a fibrin glue. In general, hydrogelsare cross-linked polymeric materials that can absorb more than 20% oftheir weight in water while maintaining a distinct three-dimensionalstructure. This definition includes dry cross-linked polymers that willswell in aqueous environments, as well as water-swollen materials. Ahost of hydrophilic polymers can be cross-linked to produce hydrogels,whether the polymer is of biological origin, semi-synthetic, or whollysynthetic. The hydrogel may be produced from a synthetic polymericmaterial. Such synthetic polymers can be tailored to a range ofproperties and predictable lot-to-lot uniformity, and represent areliable source of material that generally is free from concerns ofimmunogenicity. The matrices may include hydrogels formed from selfassembling peptides, as those discussed in U.S. Pat. Nos. 5,670,483 and5,955,343, U.S. Pub. App. No. 2002/0160471, and PCT Publication No. WO02/062969.

Properties that make hydrogels valuable in drug delivery applicationsinclude the equilibrium swelling degree, sorption kinetics, solutepermeability, and their in vivo performance characteristics.Permeability to compounds depends in part upon the swelling degree orwater content and the rate of biodegradation. Since the mechanicalstrength of a gel declines in direct proportion to the swelling degree,it is also well within the contemplation of the present invention thatthe hydrogel can be attached to a substrate so that the composite systemenhances mechanical strength. In some embodiments, the hydrogel can beimpregnated within a porous substrate, so as to gain the mechanicalstrength of the substrate, along with the useful delivery properties ofthe hydrogel.

Non-limiting examples of scaffold or matrix (sometimes referred tocollectively as “framework”) that may be used in the present inventioninclude textile structures such as weaves, knits, braids, meshes,non-wovens, and warped knits; porous foams, semi-porous foams,perforated films or sheets, microparticles, beads, and spheres andcomposite structures being a combination of the above structures.Nonwoven mats may, for example, be formed using fibers comprised of asynthetic absorbable copolymer of glycolic and lactic acids (PGA/PLA),sold under the tradename VICRYL sutures (Ethicon, Inc., Somerville,N.J.). Foams, composed of, for example,poly(epsilon-caprolactone)/poly(glycolic acid) (PCL/PGA) copolymer,formed by processes such as freeze-drying, or lyophilized, as discussedin U.S. Pat. No. 6,355,699, also may be utilized. Hydrogels such asself-assembling peptides (e.g., RAD16) may also be used. In situ-formingdegradable networks are also suitable for use in the invention (see,e.g., Anseth, K S et al. (2002) J. Controlled Release 78:199-209; Wang,D. et al., (2003) Biomaterials 24:3969-3980; U.S. Patent Publication2002/0022676 to He et al.). These in situ forming materials areformulated as fluids suitable for injection, and then may be induced toform a hydrogel by a variety of means such as change in temperature, pH,and exposure to light in situ or in vivo.

In another embodiment, the framework is a felt, which can be composed ofa multifilament yarn made from a bioabsorbable material, e.g., PGA, PLA,PCL copolymers or blends, or hyaluronic acid. The yarn is made into afelt using standard textile processing techniques consisting ofcrimping, cutting, carding and needling. In another embodiment, cellsare seeded onto foam scaffolds that may be composite structures.

In many of the abovementioned embodiments, the framework may be moldedinto a useful shape, such as that of a blood vessel. Furthermore, itwill be appreciated that umbilical cord tissue-derived cells may becultured on pre-formed, non-degradable surgical or implantable devices,e.g., in a manner corresponding to that used for preparingfibroblast-containing GDC endovascular coils, for instance (Marx, W F etal., (2001) Am. J. Neuroradiol. 22:323-333).

The matrix, scaffold or device may be treated prior to inoculation ofcells in order to enhance cell attachment. For example, prior toinoculation, nylon matrices can be treated with 0.1 molar acetic acidand incubated in polylysine, PBS, and/or collagen to coat the nylon.Polystyrene can be similarly treated using sulfuric acid. The externalsurfaces of a framework may also be modified to improve the attachmentor growth of cells and differentiation of tissue, such as by plasmacoating the framework or addition of one or more proteins (e.g.,collagens, elastic fibers, reticular fibers), glycoproteins,glycosaminoglycans (e.g., heparin sulfate, chondroitin-4-sulfate,chondroitin-6-sulfate, dermatan sulfate, keratin sulfate), geneticmaterials such as cytokines and growth factors, a cellular matrix,and/or other materials, including but not limited to, gelatin,alginates, agar, agarose, and plant gums, among other factors affectingcell survival and differentiation.

hUTC-containing frameworks are prepared according to methods known inthe art. For example, cells can be grown freely in a culture vessel tosub-confluency or confluency, lifted from the culture and inoculatedonto the framework. Growth factors may be added to the culture mediumprior to, during, or subsequent to inoculation of the cells to triggerdifferentiation and tissue formation, if desired. Alternatively, theframeworks themselves may be modified so that the growth of cellsthereon is enhanced, or so that the risk of rejection of the implant isreduced. Thus, one or more biologically active compounds, including, butnot limited to, anti-inflammatory compounds, immunosuppressants orgrowth factors, may be added to the framework for local release.

Umbilical cord tissue-derived cells, parts of umbilical cordtissue-derived cells, or cell populations comprising umbilical cordtissue-derived cells, or components of or products produced by umbilicalcord tissue-derived cells, may be used in a variety of ways to supportand facilitate the repair, regeneration, and improvement of skeletalmuscle cells and tissues, to improve blood flow, and to stimulate and/orsupport angiogenesis, especially in peripheral vascular diseasepatients. Such utilities encompass in vitro, ex vivo and in vivomethods.

In one embodiment, as discussed above, umbilical cord tissue-derivedcells can be cultured in vitro to produce biological products that areeither naturally produced by the cells, or produced by the cells wheninduced to differentiate into skeletal muscle, vascular smooth muscle,pericyte, or vascular endothelial lineages, or produced by the cells viagenetic modification. For instance, TIMP1, TPO, KGF, HGF, FGF, HBEGF,BDNF, MIP1b, MCP1, RANTES, I309, TARC, MDC, and IL-8 were found to besecreted from umbilicus-derived cells grown in Growth Medium. Inaddition, factors for endothelial progenitor cell recruitment such asVEGF, SDF-1, EPO, G-CSF, statins, estrogen, PPARγ, and CXCR4 may beproduced by umbilical cord tissue-derived cells and may be secreted intothe growth medium. Other trophic factors, as yet undetected orunexamined, for use in skeletal muscle or vascular repair andregeneration, are likely to be produced by umbilical cord tissue-derivedcells and possibly secreted into the medium.

In this regard, another embodiment of the invention features use ofumbilical cord tissue-derived cells for production of conditionedmedium, either from undifferentiated umbilical cord tissue-derived cellsor from umbilical cord tissue-derived cells incubated under conditionsthat stimulate differentiation into a skeletal muscle or vascularlineage. Such conditioned media are contemplated for use in in vitro orex vivo culture of skeletal muscle, vascular smooth muscle, pericyte, orvascular endothelial precursor cells, or in vivo to support transplantedcells comprising homogeneous populations of umbilical cordtissue-derived cells or heterogeneous populations comprising umbilicalcord tissue-derived cells and skeletal muscle, vascular smooth muscle,pericyte, or vascular endothelial progenitors, or to recruit endothelialprogenitor cells to the site of ischemic injury, for example.

Yet another embodiment comprises the use of hUTC cell lysates, solublecell fractions or components thereof, or ECM or components thereof, fora variety of purposes. As mentioned above, some of these components maybe used in pharmaceutical compositions. In other embodiments, a celllysate or ECM is used to coat or otherwise treat substances or devicesto be used surgically, or for implantation, or for ex vivo purposes, topromote healing or survival of cells or tissues contacted in the courseof such treatments. In some preferred embodiments, such preparationsmade from umbilical cord tissue-derived cells comprise FGF and HGF.

In another embodiment, umbilical cord tissue-derived cells are usedadvantageously in co-cultures in vitro to provide trophic support toother cells, in particular, skeletal muscle cells, skeletal muscleprogenitor cells, vascular smooth muscle cells, vascular smooth muscleprogenitor cells, pericytes, vascular endothelial cells, or vascularendothelium progenitor cells. In some preferred embodiments, the trophicsupport is proliferation of the cells. For co-culture, it may bedesirable for the umbilical cord tissue-derived cells and the desiredother cells to be co-cultured under conditions in which the two celltypes are in contact. This can be achieved, for example, by seeding thecells as a heterogeneous population of cells in culture medium or onto asuitable culture substrate. Alternatively, the umbilical cordtissue-derived cells can first be grown to confluence, and then willserve as a substrate for the second desired cell type in culture. Inthis latter embodiment, the cells may further be physically separated,e.g., by a membrane or similar device, such that the other cell type maybe removed and used separately, following the co-culture period. Use ofumbilical cord tissue-derived cells in co-culture to promote expansionand differentiation of skeletal muscle or vascular cell types may findapplicability in research and in clinical/therapeutic areas. Forinstance, umbilical cord tissue-derived cell co-culture may be utilizedto facilitate growth and differentiation of skeletal muscle, vascularsmooth muscle, pericytes, or vascular endothelial cells in culture, forbasic research purposes or for use in drug screening assays, forexample. Umbilical cord tissue-derived cell co-culture may also beutilized for ex vivo expansion of skeletal muscle, vascular smoothmuscle, pericyte, or vascular endothelium progenitors for lateradministration for therapeutic purposes. For example, skeletal muscle,vascular smooth muscle, pericyte, or vascular endothelium progenitorcells may be harvested from an individual, expanded ex vivo inco-culture with umbilical cord tissue-derived cells, then returned tothat individual (autologous transfer) or another individual (syngeneicor allogeneic transfer). In these embodiments, it will be appreciatedthat, following ex vivo expansion, the mixed population of cellscomprising the umbilical cord tissue-derived cells and skeletal muscle,vascular smooth muscle, pericyte, or vascular endothelium progenitorscould be administered to a patient in need of treatment. Alternatively,in situations where autologous transfer is appropriate or desirable, theco-cultured cell populations may be physically separated in culture,enabling removal of the autologous skeletal muscle, vascular smoothmuscle, or vascular endothelium progenitors for administration to thepatient.

As described in U.S. Patent Publication Nos. 2005/0058631, 2005/0054098and 2005/0058630, umbilical cord tissue-derived cells have been shown tobe effectively transplanted into the body, and to improve blood flow andreduce tissue necrosis in an accepted animal model. Those findings,along with the discoveries set forth in the present invention, supportpreferred embodiments of the invention, wherein umbilical cordtissue-derived cells are used in cell therapy for treating ischemicinjury or damage by repairing or regenerating skeletal muscle and/orvascular tissue in a peripheral vascular disease patient, or byimproving blood flow or stimulating and/or supporting angiogenesis in aperipheral vascular disease patient. In one embodiment, the umbilicalcord tissue-derived cells are transplanted into a target location in thebody, especially at or proximal to the location of the ischemic episode,where the umbilical cord tissue-derived cells can differentiate into oneor more of skeletal muscle, vascular smooth muscle, pericyte, orvascular endothelium phenotypes, the umbilical cord tissue-derived cellscan provide trophic support for skeletal muscle cell, vascular smoothmuscle cell, pericyte, or vascular endothelial cell progenitors and/orskeletal muscle cells, vascular smooth muscle cells, pericytes, orvascular endothelial cells in situ, the umbilical cord tissue-derivedcells can produce factors to recruit endothelial progenitor cells to thesite of the ischemic injury, or the umbilical cord tissue-derived cellscan exert a beneficial effect in two or more of those fashions, amongothers. Umbilical cord tissue-derived cells secrete trophic factorsincluding, but not limited to GFGFm, IL-6, IL-8, HGF, IGF-1, TPO, andthe like. Umbilical cord tissue-derived cells can aid in the recruitmentof vascular progenitor cells such as angioblasts to stimulate new bloodvessel formation.

Umbilical cord tissue-derived cells can exert trophic effects in thebody of the patient to which they are administered. For example,umbilical cord tissue-derived cells can exert trophic effects onskeletal muscle cells, vascular smooth muscle cells, vascularendothelial cells, pericytes, or progenitor cells thereof. In somepreferred embodiments, the trophic effect is the proliferation of suchcells. Umbilical cord tissue-derived cells can also induce migration ofcells in the body of the patient to which they are administered. Suchmigration can facilitate the repair, regeneration, and treatment ofperipheral vascular disease such as peripheral ischemia. For example,umbilical cord tissue-derived cells administered at or near a site ofperipheral vascular disease can induce migration of cells to the site ofperipheral vascular disease in order to repair, regenerate, or otherwisetreat the diseased tissue and its surroundings. Umbilical cordtissue-derived cells so administered can induce migration of skeletalmuscle cells, vascular smooth muscle cells, vascular endothelial cells,pericytes, or progenitor cells thereof. In preferred embodiments,umbilical cord tissue-derived cells induce migration of vascularendothelial cells and/or vascular endothelium progenitor cells to thesite, or at least near to the site of the peripheral vascular disease.In some embodiments, migration is induced or supported by FGF and/orHGF, preferably FGF and HGF expressed by the umbilical cordtissue-derived cells. Preparations made from umbilical cordtissue-derived cells, including cell lysates, subcellular fractions, andthe like, can also be used to treat peripheral vascular disease. Suchpreparations can be formulated with pharmaceutically acceptable carrierssuch as those described and exemplified herein, and administered topatients in amounts effective to treat peripheral vascular disease. Inpreferred embodiments, preparations made from umbilical cordtissue-derived cells comprise FGF and HGF.

Specific embodiments of the invention are directed to the direct repair,regeneration, replacement of, or the support of the repair,regeneration, or replacement of blood vessels for the treatment ofperipheral ischemic injury or damage.

Umbilical cord tissue-derived cells may be administered alone (e.g., assubstantially homogeneous populations) or as admixtures with othercells. As described above, umbilical cord tissue-derived cells may beadministered as formulated in a pharmaceutical preparation with a matrixor scaffold, or with conventional pharmaceutically acceptable carriers.Where umbilical cord tissue-derived cells are administered with othercells, they may be administered simultaneously or sequentially with theother cells (either before or after the other cells). Cells that may beadministered in conjunction with umbilical cord tissue-derived cellsinclude, but are not limited to, myocytes, skeletal muscle cells,skeletal muscle progenitor cells, vascular smooth muscle cells, vascularsmooth muscle progenitor cells, pericytes, vascular endothelial cells,or vascular endothelium progenitor cells, and/or other multipotent orpluripotent stem cells. The cells of different types may be admixed withthe umbilical cord tissue-derived cells immediately or shortly prior toadministration, or they may be co-cultured together for a period of timeprior to administration.

The umbilical cord tissue-derived cells may be administered with otherbeneficial drugs or biological molecules, or other active agents, suchas anti-inflammatory agents, anti-apoptotic agents, antioxidants, growthfactors, angiogenic factors, or myoregenerative or myooprotective drugsas known in the art. When umbilical cord tissue-derived cells areadministered with other agents, they may be administered together in asingle pharmaceutical composition, or in separate pharmaceuticalcompositions, simultaneously or sequentially with the other agents(either before or after administration of the other agents). The otheragents may be a part of a treatment regimen that begins either beforetransplantation and continuing throughout the course of recovery, or maybe initiated at the time of transplantation, or even aftertransplantation, as a physician of skill in the art deems appropriate.

Examples of other components that may be administered with umbilicalcord tissue-derived cells include, but are not limited to: (1) otherangiogenic factors, angiogenic drugs, or myoregenerative ormyooprotective factors or drugs; (2) selected extracellular matrixcomponents, such as one or more types of collagen known in the art,and/or growth factors, platelet-rich plasma, and drugs (alternatively,umbilical cord tissue-derived cells may be genetically engineered toexpress and produce growth factors); (3) anti-apoptotic agents (e.g.,erythropoietin (EPO), EPO mimetibody, thrombopoietin, insulin-likegrowth factor (IGF)-I, IGF-II, hepatocyte growth factor, caspaseinhibitors); (4) anti-inflammatory compounds (e.g., p38 MAP kinaseinhibitors, TGF-beta inhibitors, statins, IL-6 and IL-1 inhibitors,Pemirolast, Tranliast, REMICADE® (Centocor, Inc., Malvern, Pa.),Sirolimus, and non-steroidal anti-inflammatory drugs (NSAIDS) (such asTepoxalin, Tolmetin, and Suprafen); (5) immunosuppressive orimmunomodulatory agents, such as calcineurin inhibitors, mTORinhibitors, antiproliferatives, corticosteroids and various antibodies;(6) antioxidants such as probucol, vitamins C and E, coenzyme Q-10,glutathione, L-cysteine and N-acetylcysteine; and (6) local anesthetics,to name a few.

In one embodiment, umbilical cord tissue-derived cells are administeredas undifferentiated cells, i.e., as cultured in Growth Medium.Alternatively, umbilical cord tissue-derived cells may be administeredfollowing exposure in culture to conditions that stimulatedifferentiation toward a desired skeletal muscle, vascular smoothmuscle, pericyte, or vascular endothelium phenotype.

The cells of the invention may be surgically implanted, injected,delivered (e.g., by way of a catheter, syringe, shunt, stent,microcatheter, or pump), or otherwise administered directly orindirectly to the site of ischemic injury, damage, or distress. Routesof administration of the cells of the invention or compositions thereofinclude, but are not limited to, intravenous, intramuscular,subcutaneous, intranasal, intrathecal, intracisternal, or via syringeswith needles or catheters with or without pump devices.

When cells are administered in semi-solid or solid devices, surgicalimplantation into a precise location in the body is typically a suitablemeans of administration. Liquid or fluid pharmaceutical compositions,however, may be administered through the blood, or directly intoaffected muscle tissue (e.g., throughout a diffusely affected area, suchas would be the case for diffuse ischemic injury). The migration of theumbilical cord tissue-derived cells can be guided by chemical signals,growth factors, or calpains.

The umbilical cord tissue-derived cells or compositions and/or matricescomprising the umbilical cord tissue-derived cells may be delivered tothe site via a micro catheter, intracatheterization, or via a mini-pump.The vehicle excipient or carrier can be any of those known to bepharmaceutically acceptable for administration to a patient,particularly locally at the site at which cellular differentiation is tobe induced. Examples include liquid media, for example, DulbeccosModified Eagle's Medium (DMEM), sterile saline, sterile phosphatebuffered saline, Leibovitz's medium (L15, Invitrogen, Carlsbad, Calif.),dextrose in sterile water, and any other physiologically acceptableliquid.

Other embodiments encompass methods of treating peripheral ischemicinjury or damage by administering therapeutic compositions comprising apharmaceutically acceptable carrier and umbilical cord tissue-derivedcell cellular components (e.g., cell lysates or components thereof) orproducts (e.g., trophic and other biological factors produced naturallyby umbilical cord tissue-derived cells or through genetic modification,conditioned medium from umbilical cord tissue-derived cell culture), orumbilical cord tissue-derived cell growth medium or products purifiedfrom growth medium. In preferred embodiments, the biological factors areFGF and HGF. These methods may further comprise administering otheractive agents, such as growth factors, angiogenic factors ormyoregenerative or myoprotective drugs as known in the art.

Dosage forms and regimes for administering umbilical cord tissue-derivedcells or any of the other therapeutic or pharmaceutical compositionsdescribed herein are developed in accordance with good medical practice,taking into account the condition of the individual patient, e.g.,nature and extent of the injury or damage from the peripheral ischemicevent, age, sex, body weight and general medical condition, and otherfactors known to medical practitioners. Thus, the effective amount of apharmaceutical composition to be administered to a patient is determinedby these considerations as known in the art.

Umbilical cord tissue-derived cells have been shown not to stimulateallogeneic PBMCs in a mixed lymphocyte reaction. Accordingly,transplantation with allogeneic, or even xenogeneic, umbilical cordtissue-derived cells may be tolerated in some instances. In someembodiments, the umbilical cord tissue-derived cells themselves providean immunosuppressant effect, thereby preventing host rejection of thetransplanted umbilical cord tissue-derived cells. In such instances,pharmacological immunosuppression during cell therapy may not benecessary.

However, in other instances it may be desirable or appropriate topharmacologically immunosuppress a patient prior to initiating celltherapy. This may be accomplished through the use of systemic or localimmunosuppressive agents, or it may be accomplished by delivering thecells in an encapsulated device, as described above. These and othermeans for reducing or eliminating an immune response to the transplantedcells are known in the art. As an alternative, umbilical cordtissue-derived cells may be genetically modified to reduce theirimmunogenicity, as mentioned above.

Survival of transplanted umbilical cord tissue-derived cells in a livingpatient can be determined through the use of a variety of scanningtechniques, e.g., computerized axial tomography (CAT or CT) scan,magnetic resonance imaging (MRI) or positron emission tomography (PET)scans. Determination of transplant survival can also be done post mortemby removing the skeletal muscle or vascular tissue, and examining itvisually or through a microscope. Alternatively, cells can be treatedwith stains that are specific for skeletal muscle cells, vascular smoothmuscle cells, pericytes, or vascular endothelial cells. Transplantedcells can also be identified by prior incorporation of tracer dyes suchas rhodamine- or fluorescein-labeled microspheres, fast blue, ferricmicroparticles, bisbenzamide or genetically introduced reporter geneproducts, such as beta-galactosidase or beta-glucuronidase.

In another aspect, the invention provides kits that utilize theumbilical cord tissue-derived cells, umbilical cord tissue-derived cellpopulations, components and products of umbilical cord tissue-derivedcells in various methods for stimulating and/or supporting angiogenesis,for improving blood flow, for regenerating, repairing, and improvingskeletal muscle injured or damaged by a peripheral ischemic event, asdescribed above. Where used for treatment of damage or injury caused byan ischemic event or other scheduled treatment, the kits may include oneor more cell populations, including at least umbilical cordtissue-derived cells and a pharmaceutically acceptable carrier (liquid,semi-solid or solid). The kits also optionally may include a means ofadministering the cells, for example by injection. The kits further mayinclude instructions for use of the cells. Kits prepared for fieldhospital use, such as for military use, may include full-proceduresupplies including tissue scaffolds, surgical sutures, and the like,where the cells are to be used in conjunction with repair of acuteinjuries. Kits for assays and in vitro methods as described herein maycontain one or more of (1) umbilical cord tissue-derived cells orcomponents or products of umbilical cord tissue-derived cells, (2)reagents for practicing the in vitro method, (3) other cells or cellpopulations, as appropriate, and (4) instructions for conducting the invitro method.

The following examples describe the invention in greater detail. Theseexamples are intended to further illustrate, not to limit, aspects ofthe invention described herein.

EXAMPLE 1 Efficacy of Umbilicus-Derived Cells in the Murine HindlimbPeripheral Ischemia Model

Materials and Methods

Umbilical Cell Culture and Isolation. Umbilicus-derived cells (UDCs)were prepared as described in U.S. Patent Publications 2005/0058631 or2005/0054098. Cells were cultured to passage 10 or 11 (approximately 20to 25 population doublings) and then cryogenically preserved.

Ischemia Model Treatment Groups:

Group 1 PBS, negative control 2 Expression plasmid for vascularendothelial growth factor(pVEGF), positive control 3 cell line #1 cells,5 × 10⁵ cells total 4 cell line #1 cells, 1 × 10⁶ cells total 5 cellline #2 cells, 1 × 10⁶ cells total 6 cell line #1 cells, cultured, 1 ×10⁶ cells total cell line 1: U120304 p10, cell line 2: U072804A p11

Sample Preparation for Injection.

Cells were thawed immediately before injection (groups 3 to 5), or werecultured for 24 to 30 hours (group 6). Cells were counted and viabilitywas determined by trypan blue staining and counting on a hemocytometer.The entire dose of cells or plasmid (100 μg) was resuspended in 100 μlof PBS and loaded into a 300 μl tuberculin syringe with 27 gauge needlefor injection into the mice.

Surgery.

On day 0, acute hindlimb ischemia was surgically induced in athymic,nude mice by unilateral ligation and excision of the left iliofemerolartery. Mice were partitioned into 6 groups of at least n=8 fortreatment with UDCs or controls. Mice were randomly assigned totreatment groups for groups 1 to 5. Because group 6 was added late inthe study, randomization did not occur. In addition, schedulingconflicts precluded performing microCT/PET concurrently with theoriginal study. This analysis was performed on a group of 8 additionalanimals (4 control and 4 cultured cell 1) enrolled after the completionof the 21 day study.

Cell Injections.

One day after surgery, mice were anesthetized for laser Doppler imaginganalysis of the plantar region. While mice were still under anesthesia,cells were injected at 5 sites in the left (ischemic) limb: (1) 20 μlinto the tibilias anterior; (2) 2×20 μl into gastrocnemius; and (3) 2×20μl into rectus femoris of quadriceps bundle.

Analyses.

Laser Doppler imaging was performed at days 1, 4, 8, 14 and 21. At 21days, mice were sacrificed and tibilias anterior (TA), gastrocnemius andquadriceps muscles were excised and cryofixed for thin sectioning andimmunhistochemical staining with CD31 antibody. MicroCT/PET analysisusing fluoromethane gas to determine perfusion status of muscles wasperformed at 8 days. These mice were sacrificed immediately after andhindlimb muscles were processed for CD31 immunohistochemistry oncryofixed thin sections.

Exclusion Criteria.

Mice exhibiting severe toe necrosis at day 1 following surgery wereexcluded from the study before injections. Mice were also excluded atany time in the study due to severe necrosis (e.g., total necrosis ofthe foot) or if they experienced severe weight loss or otherwiseexhibited signs of extreme pain.

Results

The goal of these experiments was to determine if UDCs protect tissuesfrom injury in a rodent hindlimb ischemia model. This model wasperformed by creating an injury in the femoral blood flow and injectingcells in the area approximately 24 hours after the injury. The resultswere evaluated by estimating perfusion of the limbs of these animals andcomparing this to the contralateral limb that was not injured. Thetissues were also collected from these animals at the end of the studyto evaluate the vasculature and injury in the animals. This study wasalso performed with human cells in nude mice to avoid xenogenicrejection of the implanted cells.

Results presented in FIG. 1 show that the UDCs conferred a benefit onthe mice, as there was improved perfusion in the animals treated withthe cultured cells at Day 4 and 8, while blood flow was also improved inthe animals treated with the 120304 cells thawed immediately beforeinjection at Day 8. The cells 072804A did not show a benefit at any timepoint, suggesting a difference between these two lots of cells.Generally the animals showed improvement over time indicating that thisstrain of animals has some degree of native repair capability. Theseanimals were also relatively young which may be a factor in their innateregenerative capabilities.

The TA muscles were collected at the end of the study, and sections wereprobed with an anti CD31 antibody to detect vascular endothelial cells.Representative results are shown in FIG. 2. The results show that thePBS control animals presented gross necrosis and limited vasculature inthe ischemic limb, (for example mouse #26 & #43) whereas the UDC-treatedlimbs showed higher relative levels of CD31 staining and reduced levelsof necrosis. The results also suggest that the animals treated withcultured UDCs showed improved vasculature as compared to controls—(PBScontrol and in some cases, the normal (uninjured) limb). Increased CD 31staining was observed in the ischemic but treated limb as compared tothe normal limb. The animals treated with VEGF plasmid and Umb072804Ashowed similar results as PBS control.

SUMMARY

These results provide evidence that umbilical cord-derived cells can beeffective to improve blood flow and to reduce tissue necrosis in arodent hind limb ischemia model. The study included two different lotsof umbilical cells that were thawed immediately before injection, andthe results suggested differences might exist between the lots. Thecells that appeared to have some activity were also cultured forapproximately 48 hours before injection and included in anothertreatment group. These cells appeared to be the most effective and thissuggests that culturing changes the activity profile of the cells. Thehistology results also provide evidence that treatment can provideprotective effects. The results do not provide sufficient informationwith respect to the mechanism by which the UDCs exert their effects.Without intending to be bound to any particular theory or mechanism ofaction, it is believed that the cells may exert their effect bystimulating the growth of new blood vessels or protecting the muscletissue from the progression of the damage, for example, by protectionfrom apoptosis or recruitment of endogenous active agents. Additionalstudies are necessary to investigate the precise mechanism of action.

REFERENCES

-   1) Rehman, J. et al. (2004) Circulation 109:1292-1298.

EXAMPLE 2 Endothelial Network Formation Assay

Angiogenesis, or the formation of new vasculature, is necessary for thegrowth of new tissue. Induction of angiogenesis is an importanttherapeutic goal in many pathological conditions. To identify potentialangiogenic activity of the umbilical cord tissue-derived cells in vitroassays, a well-established method of seeding endothelial cells onto aculture plate coated with a biological cell culture substrate under thetradename MATRIGEL (BD Discovery Labware, Bedford, Mass.), a basementmembrane extract (Nicosia and Ottinetti (1990) In Vitro Cell Dev. Biol.26(2):119-28) was followed. Treating endothelial cells on MATRIGEL (BDDiscovery Labware, Bedford, Mass.) with angiogenic factors willstimulate the cells to form a network that is similar to capillaries.This is a common in vitro assay for testing stimulators and inhibitorsof blood vessel formation (Ito et al. (1996) Int. J. Cancer67(1):148-52). The experiments made use of a co-culture system with theumbilical cord tissue-derived cells seeded onto culture well inserts.These permeable inserts allow for the passive exchange of mediacomponents between the endothelial and the umbilical cord tissue-derivedcell culture media.

Methods & Materials

Cell Culture

Umbilical and Placental Tissue-Derived Cells.

Human umbilical cords and placenta were received and cells were isolatedas previously described (see Example 1). Cells were cultured in Growthmedium (Dulbecco's Modified Essential Media (DMEM; Invitrogen, Carlsbad,Calif.), 15% (v/v) fetal bovine serum (Hyclone, Logan Utah)), 100Units/milliliter penicillin, 100 microgram/milliliter streptomycin(Invitrogen), 0.001% (v/v) 2-mercaptoethanol (Sigma, St. Louis, Mo.)) ongelatin-coated tissue culture plastic flasks. The cultures wereincubated at 37° C. with 5% CO₂. Cells used for experiments were betweenpassages 4 and 12.

Actively growing cells were trypsinized, counted, and seeded onto COSTARTRANSWELL 6.5 millimeter diameter tissue culture inserts (Corning,Corning, N.Y.) at 15,000 cells per insert. Cells were cultured on theinserts for 48 to 72 hours in Growth medium at 37° C. under standardgrowth conditions.

Human Mesenchymal Stem Cells (hMSC).

hMSCs were purchased from Cambrex (Walkersville, Md.) and cultured inMSCGM (Cambrex). The cultures were incubated under standard growthconditions.

Actively growing MSCs were trypsinized and counted and seeded ontoCOSTAR TRANSWELL 6.5 millimeter diameter tissue culture inserts(Corning, Corning, N.Y.) at 15,000 cells per insert. Cells were culturedon the inserts for 48-72 hours in Growth medium under standard growthconditions.

Human Umbilical Vein Endothelial Cells (HUVEC).

HUVEC were obtained from Cambrex (Walkersville, Md.). Cells were grownin separate cultures in either EBM or EGM endothelial cell media(Cambrex). Cells were grown on standard tissue-cultured plastic understandard growth conditions. Cells used in the assay were betweenpassages 4 and 10.

Human Coronary Artery Endothelial Cells (HCAEC).

HCAEC were purchased from Cambrex Incorporated (Walkersville, Md.).These cells were also maintained in separate cultures in either the EBMor EGM media formulations. Cells were grown on standard tissue culturedplastic under standard growth conditions. Cells used for experimentswere between passages 4 and 8.

Endothelial Network Formation (MATRIGEL) Assays.

Culture plates were coated with MATRIGEL (BD Discovery Labware, Bedford,Mass.) according to manufacturer's specifications. Briefly, MATRIGEL (BDDiscovery Labware, Bedford, Mass.) was thawed at 4° C. and approximately250 microliters were aliquoted and distributed evenly onto each well ofa chilled 24-well culture plate (Corning). The plate was then incubatedat 37° C. for 30 minutes to allow the material to solidify. Activelygrowing endothelial cell cultures were trypsinized and counted. Cellswere washed twice in Growth medium with 2% FBS by centrifugation,resuspension, and aspiration of the supernatant. Cells were seeded ontothe coated wells at 20,000 cells per well in approximately 0.5milliliter Growth medium with 2% (v/v) FBS. Cells were then incubatedfor approximately 30 minutes to allow cells to settle.

Endothelial cell cultures were then treated with either 10 nanomolarhuman bFGF (Peprotech, Rocky Hill, N.J.) or 10 nanomolar human VEGF(Peprotech, Rocky Hill, N.J.) to serve as a positive control forendothelial cell response. Transwell inserts seeded with umbilical cordtissue-derived cells were added to appropriate wells with Growth mediumwith 2% FBS in the insert chamber. Cultures were incubated at 37° C.with 5% CO₂ for approximately 24 hours. The well plate was removed fromthe incubator, and images of the endothelial cell cultures werecollected with an Olympus inverted microscope (Olympus, Melville, N.Y.).

Results

In a co-culture system with placenta-derived cells or with umbilicalcord-derived cells, HUVEC form cell networks (data not shown). HUVECcells form limited cell networks in co-culture experiments with hMSCsand with 10 nanomolar bFGF (not shown). HUVEC cells without anytreatment showed very little or no network formation (data not shown).These results suggest that the umbilical cord tissue-derived cellsrelease angiogenic factors that stimulate the HUVEC.

In a co-culture system with placenta-derived cells or with umbilicalcord-derived cells, CAECs form cell networks (data not shown).

Table 2-1 shows levels of known angiogenic factors released by theplacental- and umbilical cord tissue-derived cells in Growth medium.Placental- and umbilical cord tissue-derived cells were seeded ontoinserts as described above. The cells were cultured at 37° C. inatmospheric oxygen for 48 hours on the inserts and then switched to a 2%FBS media and returned at 37° C. for 24 hours. Media was removed,immediately frozen and stored at −80° C., and analyzed by theSearchLight multiplex ELISA assay (Pierce Chemical Company, Rockford,Ill.). Results shown are the averages of duplicate measurements. Theresults show that the umbilical- and placental-derived cells do notrelease detectable levels of platelet-derived growth factor-bb (PDGF-bb)or heparin-binding epidermal growth factor (HBEGF). The cells do releasemeasurable quantities of tissue inhibitor of metallinoprotease-1(TIMP-1), angiopoietin 2 (ANG2), thrombopoietin (TPO), keratinocytegrowth factor (KGF), hepatocyte growth factor (HGF), fibroblast growthfactor (FGF), and vascular endothelial growth factor (VEGF).

TABLE 2-1 Potential angiogenic factors released from umbilical andplacental-derived cells. TIMP1 ANG2 PDGFBB TPO KGF HGF FGF VEGF HBEGF(pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml)Plac (P4) 91655.3 175.5 <2.0 275.5 3.0 58.3 7.5 644.6 <1.2 Plac (P11)1592832.4 28.1 <2.0 1273.1 193.3 5960.3 34.8 12361.1 1.7 Umb cord (P4)81831.7 <9.8 <2.0 365.9 14.1 200.2 5.8 <4.0 <1.2 Media alone <9.8 25.1<2.0 <6.4 <2.0 <3.2 <5.4 <4.0 <1.2Umbilical- and placental-derived cells were cultured in 24 hours inmedia with 2% FBS in atmospheric oxygen. Media was removed and assayedby the SearchLight multiplex ELISA assay (Pierce). Results are the meansof a duplicate analysis. Values are concentrations in the media reportedin picograms per milliliter of culture media. Plac: placenta derivedcells; Umb cord: umbilical cord derived cells.

Table 2-2 shows levels of known angiogenic factors released by theumbilical- and placental-derived cells. Umbilical- and placental-derivedcells were seeded onto inserts as described above. The cells werecultured in Growth medium at 5% oxygen for 48 hours on the inserts andthen switched to a 2% FBS medium and returned to 5% O₂ incubation for 24hours. Media was removed, immediately frozen, and stored at −80° C., andanalyzed by the SearchLight multiplex ELISA assay (Pierce ChemicalCompany, Rockford, Ill.). Results shown are the averages of duplicatemeasurements. The results show that the umbilical- and placental-derivedcells do not release detectable levels of platelet-derived growthfactor-bb (PDGF-BB) or heparin-binding epidermal growth factor (HBEGF).The cells do release measurable quantities of tissue inhibitor ofmetallinoprotease-1 (TIMP-1), angiopoietin 2 (ANG2), thrombopoietin(TPO), keratinocyte growth factor (KGF), hepatocyte growth factor (HGF),fibroblast growth factor (FGF), and vascular endothelial growth factor(VEGF).

TABLE 2-2 Potential angiogenic factors released from umbilical- andplacental-derived cells. TIMP1 ANG2 PDGF-BB TPO KGF HGF FGF VEGF HBEGF(pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml) (pg/ml)Plac (P4) 72972.5 253.6 <2.0 743.1 2.5 30.2 15.1 1495.1 <1.2 Plac (P11)458023.1 55.1 <2.0 2562.2 114.2 2138.0 295.1 7521.3 1.8 Umb cord (P4)50244.7 <9.8 <2.0 403.3 10.7 156.8 5.7 <4.0 <1.2 Media alone <9.8 25.1<2.0 <6.4 <2.0 <3.2 <5.4 <4.0 <1.2Umbilical- and placental-derived cells were cultured in 24 hours inmedia with 2% FBS in 5% oxygen. Media was removed and assayed by theSearchLight multiplex ELISA assay (Pierce). Results are the means of aduplicate analysis. Values are concentrations in the media reported inpicograms per milliter of culture media. Plac: placenta derived cells;Umb cord: umbilical cord derived cells.

SUMMARY

The results show that umbilical- and placental-derived cells canstimulate both human umbilical vein and coronary artery endothelialcells to form networks in an in vitro MATRIGEL (BD Discovery Labware,Bedford, Mass.) assay. This effect is similar to that seen with knownangiogenic factors in this assay system. These results suggest that theumbilical- and placental-derived cells are useful for stimulatingangiogenesis in vivo.

EXAMPLE 3 Effect if hUTCs on the In Vitro Proliferation and Migration ofEndothelial Cells

Studies were undertaken to determine the effects of human umbilicaltissue-derived cells (hUTCs) on the proliferation and migration ofendothelial cells in vitro. These effects were examined by co-culturinghUTCs and endothelial cells and by incubating cultures of humanumbilical vein endothelial cells (HUVECs) with hUTC lysates. The resultspresented here show that hUTCs induce increases in proliferation andmigration of endothelial cells. Furthermore, the data suggest that theseeffects are mediated, in part, by fibroblast growth factor (FGF) andhepatocyte growth factor (HGF).

Materials and Methods

Cell Culture

Cryopreserved human umbilical tissue-derived cells (hUTCs) lot#120304were thawed at passage 8-9 and seeded onto gelatin-coated flasks andcultured in Hayflick growth media (DMEM—low glucose (Gibco, catalognumber11885-084), 15% v/v fetal bovine serum (FBS, Hyclone, catalognumber SH30070.03), 0.001% v/v beta-mercaptoethanol (Sigma, catalognumber M7154), and 50 U/ml penicillin and 50 micrograms/ml streptomycin(Gibco, catalog number 3810-74-0)). For studies detailed here, cellsused were at passage 10 or 11. Human umbilical vein endothelial cells(HUVECs, catalog number C2517A), human coronary artery endothelial cells(HCAECs, catalog number CC2585), and human iliac artery endothelialcells (HIAECs, catalog number CC2545) were obtained from Cambrex andwere cultured in endothelial growth medium (EGM-2MV, catalog number3202) according to manufacturer's recommendations. Human mesenchymalstem cells (MSCs, catalog number PT-2501) were also purchased fromCambrex and were maintained in mesenchymal stem cell growth medium(MSCGM, catalog number PT-3001) according to manufacturer'srecommendations. Human dermal fibroblasts (CCD9) were from ATCC and weremaintained in DMEM/F12 media containing 10% FBS and 1 U/mlpenicillin-streptomycin.

For routine passage, cells were washed once with phosphate bufferedsaline (PBS, Invitrogen, catalog number 14190) and detached bytrypsinization (0.25% trypsin-EDTA, Invitrogen, catalog number25200-056). Cells were counted using a Guava® instrument (GuavaTechnologies, Hayward, Calif.) and seeded at a density of 5000cells/cm². Cells were routinely passaged every 3-4 days.

Growth Factors and Antibodies

Recombinant human basic fibroblast growth factor (bFGF, catalog number100-18B) and recombinant human hepatocyte growth factor (HGF, catalognumber 100-39) were from Peprotech and recombinant human vascularendothelial growth factor (VEGF, catalog number 293-VE) was from R and DSystems. Antibodies to bFGF (catalog number ab11937), HGF (catalognumber ab10678), and VEGF (catalog number ab9570) were purchased fromAbcam (Cambridge, Mass.).

Preparation of Cell Lysate

Cell lysates were prepared from frozen hUTC lot#120304 cell pellets fromprevious grow-ups. Briefly, hUTC lot#120304 were cultured for 4 days,harvested by trypsinization, and pelleted by centrifugation. Cells werethen washed with PBS 3 times and resuspended in PBS at 1×10⁷ cells/ml.Aliquots of 1 ml suspensions were placed into 1.5 ml sterile siliconizedmicrocentrifuge tubes and centrifuged at 300 rcf for 5 minutes. PBS wasaspirated and cell pellets stored at −80° C. until use.

To prepare cell lysates, tubes containing cell pellets were immersed inliquid nitrogen (LN2) for 60 seconds and then immediately immersed in a37° C. water bath for 60 seconds or until thawed but not longer than 3minutes. This step was repeated 3 times. Following this step, thefreeze-thawed samples were centrifuged at 13000 rcf at 4° C. for 10minutes and then placed on ice. The supernatant was carefully removedand transferred to a fresh sterile siliconized 1.5 ml tube. Thecentrifugation step was repeated 3 times and the resulting supernatantpooled. Protein concentration was determined using the microassayprotocol of the Quickstart Bradford protein assay kit (Bio-rad, catalognumber 500-0201).

Measurement of Cell Proliferation

Cells were harvested and plated directly into the indicated mediaformulation at a concentration of 5000 cells/cm². For co-cultureexperiments, 24-well transwells (Corning catalog number 3413) were usedwith endothelial cells plated on the bottom of the well (10,000cells/well) and hUTCs, MSCs, or fibroblasts plated inside the transwellinserts (1650 cells/transwell inserts). At the indicated time periods,inserts containing hUTCS, MSCs, or fibroblasts were removed anddiscarded. Endothelial cells were harvested by adding 90 μl of trypsinto each well. Cells were released by pipetting up and down and thentransferred to a clean 96-well plate. Trypsin was inhibited by theaddition of 90 μl of media. Cells were stained by addition of 20 μl ofstaining solution (18 μl of media+1 μl Guava Viacount Flex Reagent+1 μlof DMSO) and quantitated using a Guava® instrument (Guava Technologies,Hayward, Calif.).

For studies on the effect of hUTC lot#120304 cell lysate on theproliferation of HUVECs, HUVECs were seeded onto 24-well tissue culturedishes at a density of 10,000 cells/well in EGM-2MV media for 8 hours.Cells were then serum-starved by overnight incubation in 0.5 ml ofEGM-2MV media containing 0.5% FBS and without growth factors.Afterwards, FBS, freshly prepared hUTC lot#120304 cell lysate containing62.5 μg or 125 μg of protein, and neutralizing antibodies to FGF (7μg/ml) or HGF (1 μg/ml) were added. After 4 days of culture, cells wereharvested and counted using a Guava® instrument.

For studies on the potential mechanisms of hUTC-mediated increase inendothelial cell proliferation, neutralizing antibodies to FGF (7ng/ml), HGF (1 ng/ml), and VEGF (1 ng/ml) were included in co-culturesof HUVECs and HCAECs with hUTCs. The antibodies were added to the cellculture media when the cells were initially plated. After 7 days ofco-culture, cells were harvested and counted using a Guava® instrument.

Assessment of Cell Migration

For measurement of cell migration, a 6-well transwell (Corning catalognumber 3428) set-up was used. Cells were seeded directly into theindicated media formulation at a density of 5000 cells/cm². Endothelialcells were seeded inside the transwell inserts (23,000 cells/transwellinsert) and hUTC lot#120304 or MSCs plated onto the bottom of the well(48,000 cells/well). Migration was assessed after 7 days of co-cultureby counting the number of cells on the underside of the transwell.Briefly, transwells were transferred to a clean well and washed oncewith PBS. Cells from the underside of the well were harvested by addingtrypsin to the bottom of the well. Trypsin was inhibited by the additionof complete growth media and cells collected by centrifugation. Cellswere then resuspended in 25 μl of media and 20 μl of this used to obtaincell counts using a Guava® instrument.

For studies on the potential mechanisms of hUTC-mediated increase inendothelial cell migration, neutralizing antibodies to FGF (7 ng/ml) andHGF (1 ng/ml) were included in co-cultures of HUVECs and HCAECs withhUTC lot#120304. The antibodies were added to the cell culture mediawhen the cells were initially plated. After 7 days of co-culture, cellsthat were on the underside of the transwell insert were harvested andcounted using a Guava® instrument.

Results

Effect of hUTCs on Proliferation of Endothelial Cells

A co-culture system was utilized to study the effects of hUTCs on theproliferation of endothelial cells. This was performed using a transwellset-up with endothelial cells plated on the bottom of a 24-well tissueculture dish and hUTCs plated inside the transwell inserts. In theseexperiments, two different media formulations were used (mediacomposition detailed in Materials and Methods): (1) Hayflick 80%+EGM-2MV20% (H80) or (2) Hayflick 50%+EGM-2MV 50% (H50). After 6 or 7 days ofco-culture, the transwell inserts were removed, endothelial cellsharvested by trypsinization, and counted using the Guava® instrument.

The effect of hUTC lot#120304 on the proliferation of endothelial cellscultured in H80 compared with H50 is shown in FIG. 1. The proliferationof HUVECs maintained in H50 was higher than those kept in H80 (FIG. 1A)while HCAECs and HIAECs exhibited similar growth in these co-culturemedia formulations (FIG. 1B and FIG. 1C). In both media formulations,co-culture of endothelial cells with hUTC lot#120304 resulted insignificant increases in cell number after 7 days. All subsequentco-culture studies of hUTCs and endothelial cells were performed in theHayflick 50%+EGM-2MV 50% (H50) media formulation.

MSCs and fibroblasts were also tested in co-cultures with endothelialcells to determine whether other cell types have the ability toinfluence the proliferation of endothelial cells. As shown in FIG. 1A,there was no difference in the proliferation of HUVECs in co-culturemedia (H50 or H80) and those that were co-cultured with MSCs or withfibroblasts. The same was true of HCAECs (FIG. 1B) and HIAECs (FIG. 1C)where co-culture with hUTC lot#120304 resulted in increased cellproliferation while no differences can be observed between cells inco-culture media (H50 or H80) and those that were co-cultured with MSCs.

To investigate the potential mechanisms of hUTC-mediated increase inendothelial cell proliferation, neutralizing antibodies to FGF (7mg/ml), HGF (1 mg/ml), and VEGF (1 μg/ml) were included in co-culturesof HUVECs and HCAECs with hUTCs. Results in FIGS. 2A to 2D show that inboth HUVECs and HCAECs the addition of neutralizing antibodies to FGFand HGF reduced the increase in cell number induced by hUTC lot#120304.At the concentrations that were used for these studies, theseneutralizing antibodies blocked proliferation of HUVECs induced by thegrowth factors (FIGS. 2A and 2B). It is interesting to note that aneutralizing antibody to VEGF did not have a significant effect on thecell proliferation induced by co-culture of both HUVECs (FIGS. 2A and2B) and HCAECs (FIGS. 2C and 2D) with hUTC lot#120304. In separatestudies, the proliferation of hUTC lot#120304 was not affected by theaddition of neutralizing antibodies to FGF and VEGF to the culture media(data not shown).

Effect of hUTC Lot#120304 Cell Lysate on Proliferation of HUVECs

Studies were also conducted to determine the effect of cell lysate onthe proliferation of HUVECs. HUVECs were seeded onto 24-well plates inEGM-2MV media for 8 h at a density of 5000 cells/cm². The cells werethen serum-starved by an overnight incubation in 0.5 ml of EGM-2MV mediacontaining 0.5% fetal bovine serum (FBS) and without growth factors.Following the incubation, varying concentrations of freshly preparedhUTC lot#120304 cell lysate were added. In some instances, FGF, HGF, andneutralizing antibodies were also included. After 4 days of culture,HUVECs were harvested and counted using a Guava® instrument.

FIG. 3 shows that the addition of cell lysates led to an increase inHUVECs cell number compared to cells kept in low serum (0.5% FBS) andthe increase in cell number was proportional to the amount of added celllysate. The lower concentration of cell lysate used (62.5 mg/ml)resulted in a cell number comparable to cells incubated in optimal mediacondition (10% FBS). Furthermore, the addition of a neutralizingantibody to either FGF or HGF moderated the increase in cell numberinduced by the 2 different concentrations of cell lysate. These resultsare consistent with the results obtained in co-cultures of HUVECs withhUTC lot#120304.

Effect of hUTCs on Migration of Endothelial Cells

The migration of endothelial cells was assessed by determining thenumber of cells that have moved through a transwell membrane (poresize=8 microns). The responder cells, endothelial cells, were seededonto 6-well transwell inserts and hUTCs were plated on the bottom of thewell. After a period of co-culture, cells that were on the underside ofthe transwell were harvested and counted. FIG. 4A shows the migration ofHUVECs that were co-cultured with hUTCs and MSCs. hUTC lot#120304induced the movement of HUVECs to the underside of the transwell whileMSCs did not (FIG. 4A). The same result was observed with HCAECs whereco-culture with hUTC lot#120304 resulted in more cells migrating throughthe transwell relative to media control (FIG. 4B).

The effect of hUTC lot#120304 on the migratory behavior of HUVECs andHCAECs was further tested with the use of neutralizing antibodies to FGFand HGF. As shown in FIG. 5A, these antibodies reduced the migration ofHUVECs induced by hUTC lot#120304. In co-cultures of HCAECs with hUTClot#120304, a neutralizing antibody to HGF blocked hUTClot#120304-mediated increase in cell migration while a neutralizingantibody to FGF did not (FIG. 5B).

SUMMARY

The results outlined here describe the effects of hUTCs on theproliferative and migratory behavior of endothelial cells in vitro. Thestudies were performed using co-cultures of hUTC lot#120304 andendothelial cells or direct incubation of endothelial cells with celllysate prepared from hUTC lot#120304.

For studies of proliferation, the effects of hUTC lot#120304 were testedand three endothelial cell types from different vascular beds were usedas responder cells. Co-culture with hUTCs resulted in enhancedproliferation of endothelial cells. Co-culture with MSCs or fibroblastsresulted in cell numbers comparable to media controls. The proliferativeresponse of HUVECs to hUTC lot#120304 was dampened by the addition ofneutralizing antibodies to FGF and HGF, but not by neutralizing antibodyto VEGF. This implies that the induction of proliferation by hUTClot#120304 is mediated by FGF and HGF. It is worth noting thatincubation of HUVECs with hUTC lot#120304 lysate mirrored the effectobserved with co-cultures.

Migration was quantitated by counting the number of cells that were onthe underside of a transwell and both HUVECs and HCAECs were used asresponder cells. Unlike the studies with proliferation, the migratoryresponses of these cells are slightly different. HUTC lot#120304 inducedthe migration of both HUVECs and HCAECs. MSCs did not induce themigration of HUVECs suggesting specificity of this response to hUTCs.Antibodies to FGF and HGF negated the effect of hUTC lot#120304 on themigration of HUVECs while only antibody to HGF affected the migration ofHCAECs suggesting differences between the two endothelial cell types.

In summary, the data show that hUTCs induce proliferation and migrationof endothelial cells in vitro. The use of neutralizing antibodiesimplicates both FGF and HGF in these observed effects. However, otherfactors may also be involved in the proliferative and migratory behaviorof endothelial cells.

EXAMPLE 4 Telomerase Expression in Umbilical-Derived Cells

Telomerase functions to synthesize telomere repeats that serve toprotect the integrity of chromosomes and to prolong the replicative lifespan of cells (Liu, K, et al., PNAS, 1999; 96:5147-5152). Telomeraseconsists of two components, telomerase RNA template (hTER) andtelomerase reverse transcriptase (hTERT). Regulation of telomerase isdetermined by transcription of hTERT but not hTER. Real-time polymerasechain reaction (PCR) for hTERT mRNA thus is an accepted method fordetermining telomerase activity of cells.

Cell Isolation.

Real-time PCR experiments were performed to determine telomeraseproduction of human umbilical cord tissue-derived cells. Human umbilicalcord tissue-derived cells were prepared in accordance the examples setforth above. Generally, umbilical cords obtained from National DiseaseResearch Interchange (Philadelphia, Pa.) following a normal deliverywere washed to remove blood and debris and mechanically dissociated. Thetissue was then incubated with digestion enzymes including collagenase,dispase and hyaluronidase in culture medium at 37° C. Human umbilicalcord tissue-derived cells were cultured according to the methods setforth in the examples above. Mesenchymal stem cells and normal dermalskin fibroblasts (cc-2509 lot #9F0844) were obtained from Cambrex,Walkersville, Md. A pluripotent human testicular embryonal carcinoma(teratoma) cell line nTera-2 cells (NTERA-2 cl.D1), (see, Plaia et al.,Stem Cells, 2006; 24(3):531-546) was purchased from ATCC (Manassas, Va.)and was cultured according to the methods set forth above.

Total RNA Isolation.

RNA was extracted from the cells using RNeasy® kit (Qiagen, Valencia,Calif.). RNA was eluted with 50 microliters DEPC-treated water andstored at −80° C. RNA was reverse transcribed using random hexamers withthe TaqMan® reverse transcription reagents (Applied Biosystems, FosterCity, Calif.) at 25° C. for 10 minutes, 37° C. for 60 minutes and 95° C.for 10 minutes. Samples were stored at −20° C.

Real-Time PCR.

PCR was performed on cDNA samples using the Applied BiosystemsAssays-On-Demand™ (also known as TaqMan® Gene Expression Assays)according to the manufacturer's specifications (Applied Biosystems).This commercial kit is widely used to assay for telomerase in humancells. Briefly, hTert (human telomerase gene (Hs00162669) and humanGAPDH (an internal control) were mixed with cDNA and TaqMan® UniversalPCR master mix using a 7000 sequence detection system with ABI prism7000 SDS software (Applied Biosystems). Thermal cycle conditions wereinitially 50° C. for 2 minutes and 95° C. for 10 minutes followed by 40cycles of 95° C. for 15 seconds and 60° C. for 1 minute. PCR data wasanalyzed according to the manufacturer's specifications.

Human umbilical cord tissue-derived cells (ATCC Accession No. PTA-6067),fibroblasts, and mesenchymal stem cells were assayed for hTert and 18SRNA. As shown in Table 4-1, hTert, and hence telomerase, was notdetected in human umbilical cord tissue-derived cells.

TABLE 4-1 hTert 18S RNA Umbilical cells (022803) ND + Fibroblasts ND +ND—not detected; + signal detected

Human umbilical cord tissue-derived cells (isolate 022803, ATCCAccession No. PTA-6067) and nTera-2 cells were assayed and the resultsshowed no expression of the telomerase in two lots of human umbilicalcord tissue-derived cells while the teratoma cell line revealed highlevel of expression (Table 4-2).

TABLE 4-2 hTert GAPDH Cell type Exp. 1 Exp. 2 Exp. 1 Exp. 2 hTert normnTera2 25.85 27.31 16.41 16.31 0.61 022803 — — 22.97 22.79 —

Therefore, it can be concluded that the human umbilical tissue-derivedcells of the present invention do not express telomerase.

EXAMPLE 5 Efficacy of hUTC Transplantation in a Murine Model of HindlimbIschemia

Previous data demonstrated that systemic administration of hUTCsignificantly improved blood flow at 5 and 10 days post-treatment inmice with unilateral hindlimb ischemia. In addition, a side-by-sidecomparative study showed that systemic (intravenous) injection of hUTCresulted in more significant restoration of blood flow compared withlocal (intramuscular) injection.

This example evaluates the efficacy of intramuscular injection of hUTCand hUTC in fibrin glue in a mouse model of peripheral hindlimb ischemia(unilateral hindlimb ischemia model) Immunocompromised nude and NOD/scidIL2rγ^(−/−) (NSG) strains of mice were used.

Animal Model & Description

For the studies in this example, comparisons were made between nude miceand NSG mice.

The NSG mouse strain has generated interest for xenotransplantationstudies because of its multiple immunological defects including absenceof mature lymphocytes, T cells, B cells, and NK cells. These animalssurvive longer than 6 months and do not develop thymic lymphomas evenafter sublethal irradiation (Ito M. et al. (2002) Blood. 100: 3175-82).

Unilateral hindlimb ischemia was created in these mice. Briefly, animalswere anesthetized by isoflurane inhalation. An incision was made at themidline of the left hindlimb. The femoral artery and its branches wereligated, beginning from the inguinal ligament to the bifurcation ofsaphenous and popliteal arteries. The regions between the ligatures wereexcised and the incisions were closed with 5-0 silk Vicryl sutures(Ethicon).

Cells and Fibrin Glue

Frozen cell suspensions were provided by shipment in a dry shipper. Oncereceived, the cells were transferred to liquid nitrogen for long-termstorage. Cells were thawed immediately before injection. Cells werecounted and viability was determined by trypan blue staining andcounting on a hemocytometer. The entire dose was resuspended in PBS andloaded into a 0.3 ml tuberculin syringe with 28 gauge needle forinjection.

Fibrin glue (EVICEL® Fibrin sealant (Human), Omrix Pharmaceuticals) wasused for these studies. The components were thawed prior to use anddiluted to a final concentration of 16-24 IU/ml of thrombin and39.3-60.7 mg/ml for BAC2 (fibrinogen). Stock solutions of thrombin(stock concentration of approximately 800-1200 IU/ml) and BAC2(fibrinogen) (stock concentration of approximately 55 to 85 mg/ml) werediluted 1:50 for thrombin and 1:1.4 for BAC2, respectively.

Study Design

A total of forty-eight (48) nude mice (6 to 8-weeks old) and forty-eight(48) NOG/SCID (NSG) mice (6 to 11-weeks old), matched by date of birth,were randomized into the groups as detailed in Table 5-1 below.

TABLE 5-1 Endpoint Testing (Days Post-Injury) Grp Test # of Cell BloodFlow Capillary # Animal Animals Test Material Dose Necrosis by LDIdensity 1 Nude 12 hUTC vehicle N/A 1-7 1, 7, 14, 21, 7 and 28 and 28 2Nude 12 hUTC 1 × 10⁶ 1-7 1, 7, 14, 21, 7 and 28 and 28 3 Nude 12Saline + Fibrin N/A 1-7 1, 7, 14, 21, 7 and 28 and 28 4 Nude 12 Saline +Fibrin + hUTC 1 × 10⁶ 1-7 1, 7, 14, 21, 7 and 28 and 28 5 NSG 12 hUTCVehicle N/A 1-7 1, 7, 14, 21, 7 and 28 and 28 6 NSG 12 hUTC 1 × 10⁶ 1-71, 7, 14, 21, 7 and 28 and 28 7 NSG 12 Saline + Fibrin N/A 1-7 1, 7, 14,21, 7 and 28 and 28 8 NSG 12 Saline + Fibrin + hUTC 1 × 10⁶ 1-7 1, 7,14, 21, 7 and 28 and 28

Endpoint Testing was conducted by measuring the following parameters:Evaluation of blood flow by laser Doppler Imaging on days 1, 7, 14, 21and 28; assessment of capillary density by CD31 staining on day 7 (3animals from each group) and day 28.

Method

One day after creation of unilateral hindlimb ischemia, vehicle, hUTC invehicle, fibrin glue, or hUTC in fibrin glue were injected into theischemic hindlimb muscle.

For hUTC injections, the specified number of hUTC in vehicle or hUTC infibrin glue was injected into the ischemic hindlimb muscle. There werethree (3×20 μL) injections into the upper limbs and two (2×20 μL) intothe lower limbs for a total dose of 100 μl. Control animals receivedvehicle in the same manner as the cells.

For each injection of hUTC in fibrin glue, cells were resuspended inthrombin (final concentration of 16 to 24 IU/ml). BAC2 (fibrinogen;final concentration of 39.3 to 60.7 mg/ml) was aliquoted into a separateeppendorf tube.

Immediately prior to injection, hUTC in thrombin were transferred intothe tube containing BAC2, mixed, and drawn into a 0.3 ml tuberculinsyringe (with 28 gauge needle) and injected into the mouse hindlimb. The100 μL was delivered in five 20 μl intramuscular (IM) injections-3injections into the upper hindlimb and 2 into the lower hindlimb.Control animals received fibrin glue delivered in the same manner as thecells.

Statistical Analysis

Data are expressed as mean±standard error of the mean. Comparisonsbetween groups were performed with a two-tailed Student's t test.

Evaluation of Blood Flow

Blood perfusion in mice hindlimbs was evaluated using laser Dopplerimaging with a Moor LDI device. Animals were anesthetized by isofluraneinhalation and will be placed on a heating pad set at 37° C. Toestablish baseline ischemia, blood perfusion data in plantar region ofboth hindlimbs was collected at 24 hours after creation of injury.Serial perfusion assessment was performed at days 7, 14, 21 and 28. Datais reported as a ratio of perfusion values in the left (ischemic) versusright (non-ischemic) limbs.

Results and Analysis

Laser Doppler Perfusion Imagining

Laser Doppler perfusion data (expressed as percentage of perfusion inthe ischemic left limb compared to the non-ischemic control right limb)for NSG mice is shown in FIG. 6 and Table 5-2 (below). The largesttreatment effect was observed with hUTC delivered in fibrin matrix;relative perfusion in these mice was nearly double the fibrin controlgroup by 21 days (40.3±2.43 vs. 22.6±2.34). At 21 and 28 days thiseffect was significantly greater than both control groups (P<0.001) aswell as the group which received hUTC delivered in vehicle alone(P<0.05). The effect of hUTC delivered in vehicle on relative perfusionwas 27% greater than control at 28 days (P<0.05). At this time pointrelative perfusion in the ischemic limb of NSG mice treated with hUTC invehicle alone was 30.0±2.3 compared to 23.7±1.6 for mice treated withonly vehicle.

TABLE 5-2 Means ± sems for relative perfusion values in NSG mice. DayAgent 1 7 14 21 28 vehicle 16.5 ± 0.9 25.4 ± 1.7 27.5 ± 1.9 25.6 ± 1.823.7 ± 1.3 hUTC 15.7 ± 1.1 30.8 ± 3.3 30.6 ± 3.1 31.7 ± 3.1 30.0 ± 2.3saline + 17.0 ± 1.1 26.5 ± 2.4 24.6 ± 2.3 22.6 ± 2.3 22.5 ± 2.0 fibrinFibrin + 14.9 ± 1.2 29.9 ± 3.4 39.6 ± 7.5 40.3 ± 2.4 41.8 ± 4.3 hUTCAverage ± sem

Perfusion data for nude mice is shown in FIG. 7 and Table 5-3. Treatmentwith hUTC in fibrin significantly (P<0.05) increased perfusion in theischemic limb at days 14 (53.9±4.7) and 21 (53.4±3.2) compared to fibrinonly treated controls (39.2±1.7 and 40.9±3.7, respectively). The effectof cells in fibrin trended higher at 28 days (52.0±5.8) compared tocontrol (40.8±4.3) but was not significant due to a large deviation inmeasurements between animals. Local delivery of hUTC in vehicle onlytrended toward enhanced perfusion at 21 days (64.0±6.3 vs. 43.7±7.4 forthe control) and significantly (P<0.05) enhanced perfusion by 28 days(52.0±3.5 vs. 40.8±4.9). There was not a significant difference betweeneffects with hUTC delivered in fibrin or vehicle only.

TABLE 5-3 Means ± sems for relative perfusion values in nude mice. DayAgent 1 7 14 21 28 vehicle 13.9 ± 1.1  32.0 ± 5.1 40.6 ± 1.7 43.7 ± 7.447.1 ± 4.9 hUTC 13.7 ± 0.6  38.4 ± 5.1 46.1 ± 3.0 64.0 ± 6.3 57.0 ± 3.5saline + 14.5 ± 0.84 29.9 ± 3.5 39.2 ± 2.7 40.1 ± 3.7 40.8 ± 4.3 fibrinFibrin + 13.4 ± 0.69 33.0 ± 3.7 54.9 ± 4.7 53.4 ± 3.2 52.0 ± 5.8 hUTCAverage ± sem

These data indicate that in both NSG and nude mouse strains hUTCdelivered locally by IM injection had early effects when admixed infibrin carrier. In NSG mice the sustained effect was significantly morepronounced than delivery of cells in vehicle alone.

CONCLUSION

Direct intramuscular administration of hUTC 1 day after creatingischemia enhanced reperfusion of ischemic muscles in both NSG and nudemice. Delivery of the cells in a fibrin matrix to NSG mice appeared toproduce a response which was superior to delivery of cells in vehiclealone. Animals treated with direct intramuscular administration of hUTCin a murine hindlimb model of peripheral ischemia showed an enhancedreperfusion of ischemic limbs in both NSG and nude mice. However,animals that were treated with hUTC in fibrin glue exhibited a moresignificant and sustained response compared to delivery of cells invehicle alone in the NSG mice.

EXAMPLE 6 Efficacy of hUTC Transplantation in the NOD/Scid IL2rγ^(−/−)Mouse Model of Peripheral Limb Ischemia: Dose and Route ofAdministration Studies

This study evaluated the efficacy of hUTC in a mouse model of peripheralhindlimb ischemia (unilateral hindlimb ischemia model). For this study,the NOD/scid IL2rγ^(−/−) (NSG) strain of mice was used. The effect onrestoration of blood flow was assessed when hUTC were delivered (1)locally (intramuscular) with vehicle, (2) locally (intramuscular) withfibrin glue, or (3) systemically (intravenous). The study also assessedthe effect of hUTC administered intramuscularly at different doses withor without fibrin glue, on restoration of blood flow.

Materials and Methods

Animal Model & Description

NSG mice were used. The NSG mouse strain has generated interest forxenotransplantation studies because of its multiple immunologicaldefects including absence of mature lymphocytes, T cells, B cells, andNK cells. These animals survive longer than 6 months and do not developthymic lymphomas even after sublethal irradiation (Ito M. et al. (2002)Blood. 100: 3175-82).

Unilateral hindlimb ischemia was created in these mice. Briefly, animalswere anesthetized by isoflurane inhalation. An incision was made at themidline of the left hindlimb. The femoral artery and its branches wereligated, beginning from the inguinal ligament to the bifurcation ofsaphenous and popliteal arteries. The region between the ligatures wasexcised and the incision was closed with 5-0 silk Vicryl sutures.

Cells and Fibrin Glue

Cryopreserved hUTC were thawed immediately before injection. Cells werecounted and viability was determined by trypan blue staining andcounting on a hemocytometer. The entire dose was resuspended in eithervehicle or fibrin glue and loaded into a 0.3 ml tuberculin syringe with28 gauge needle for injection.

Fibrin glue (EVICEL® Fibrin sealant [Human], Omrix Pharmaceuticals) wasused. The components were thawed prior to use and diluted to a finalconcentration of 16 to 24 IU/ml of thrombin and 39.3 to 60.7 mg/ml forBAC2. Stock solutions of thrombin (stock concentration of approximately800-1200 IU/ml) and BAC2 (fibrinogen) (stock concentration ofapproximately 55 to 85 mg/ml) were provided and diluted 1:50 forthrombin and 1:1.4 for BAC2, respectively.

Study Design

NSG mice (6 to 11 weeks old), matched by date of birth, were randomizedinto the groups as detailed in Table 6-1 below:

TABLE 6-1 Test Total Cells Blood Flow Group #/Group Material DeliveredROA by LDI 1 12 Vehicle N/A IM 1, 7, 14, 21, and 28 2 12 hUTC   1 × 10⁶IM 1, 7, 14, 21, and 28 3 12 hUTC 0.5 × 10⁶ IM 1, 7, 14, 21, and 28 4 12Vehicle + N/A IM 1, 7, 14, 21, Fibrin and 28 5 12 Vehicle +   1 × 10⁶ IM1, 7, 14, 21, Fibrin + and 28 hUTC 6 12 Vehicle + 0.5 × 10⁶ IM 1, 7, 14,21, Fibrin + and 28 hUTC 7 12 Vehicle + 0.25 × 10⁶  IM 1, 7, 14, 21,Fibrin + and 28 hUTC 8 12 Vehicle + 0.125 × 10⁶  IM 1, 7, 14, 21,Fibrin + and 28 hUTC 9 12 Vehicle N/A IV 1, 7, 14, 21, and 28 10 12 hUTC  1 × 10⁶ IV 1, 7, 14, 21, and 28

One day after creation of unilateral hindlimb ischemia, hUTC wereinjected either systemically or locally. For systemic injections, thespecified number of hUTC in 100 μL of vehicle was administered throughthe tail vein using a 0.3 cc insulin syringe and a 28-gauge needle. Cellinjections were performed over a period of approximately 1 minute.Control animals received vehicle only.

For local injections, the specified number of hUTC in vehicle or hUTC infibrin glue was injected into the ischemic hindlimb muscle. Injectionswere made into 5 sites; each delivered 20 μl intramuscular (IM)injections. There were three injections (3×20 μl) injections into theupper limbs and two (2×20 μl) into the lower limbs for a total dose of100 μL. Control animals received vehicle in the same manner as thecells.

For each injection of hUTC in fibrin glue, cells were resuspended inthrombin (final concentration of 16 to 24 IU/ml). BAC2 (fibrinogen;final concentration of 39.3 to 60.7 mg/ml) was aliquoted into a separateeppendorf tube. Immediately prior to injection, hUTC in thrombin weretransferred into the tube containing BAC2, mixed, and drawn into a 0.3ml tuberculin syringe (with 28 gauge needle) and injected into the mousehindlimb. The 100 μl dose was delivered in five 20 μl intramuscular (IM)injections-3 injections into the upper hindlimb and 2 into the lowerhindlimb. Control animals received fibrin glue delivered in the samemanner as the cells.

Evaluation of Blood Flow

Blood perfusion in mice hindlimbs was evaluated using laser Dopplerimaging with a Moor LDI device. Animals were anesthetized by isofluraneinhalation and were placed on a heating pad set at 37° C. To establishbaseline ischemia, blood perfusion data in plantar region of bothhindlimbs was collected at 24 hours after creation of injury. Serialperfusion assessment was performed at days 7, 14, 21 and 28 post-injury.Data is reported as a ratio of perfusion values in the left (ischemic)versus right (non-ischemic) limbs.

Results

The mean (±sem) values for relative perfusion in the ischemic limbs foreach group are displayed in Table 6-2 (shown below). Two-way ANOVAstatistical analysis was conducted on the three sets of data (e.g., IM(no fibrin), IM with fibrin and IV (no fibrin)) using a 5% significancelevel. Overall effects of time and treatment were evaluated. There was asignificant effect (P<0.01) of treatment and time in all groups. ABonferroni post-test was performed to compare all groups to control andeach other within each set (e.g., IM, IM with fibrin and IV).

TABLE 6-2 Summary of laser Doppler imaging data. Day 1 7 14 21 28 GroupTreatment Cell Dose ROA mean sem mean sem mean sem mean sem mean sem 1Vehicle N/A IM 11.4 1.0 22.8 2.2 25.4 1.9 26.8 2.8 28.1 3.3 2 hUTC   1 ×10⁶ IM 11.9 0.9 24.4 2.0 35.1 5.4

5.3

5.8 3 hUTC 0.5 × 10⁶ IM 12.4 1.3 26.7 2.4 26.7 2.0 35.3 4.0 36.7 3.1 4Vehicle + Fibrin N/A IM 11.8 1.8 25.3 1.9 23.7 2.7 17.8 1.4 24.1 3.7 5Vehicle + Fibrin + hUTC   1 × 10⁶ IM 11.1 1.0 26.7 2.4 35.8 6.0

1.8

7.6 6 Vehicle + Fibrin + hUTC 0.5 × 10⁶ IM 11.8 0.8 28.1 3.6 34.8 2.8

6.1 38.5 6.5 7 Vehicle + Fibrin + hUTC 0.25 × 10⁶  IM 10.3 0.8 25.5 1.732.1 3.7

7.3 35.4 6.3 8 Vehicle + Fibrin + hUTC 0.125 × 10⁶  IM 11.6 1.2 28.6 1.628.7 2.6

5.7 39.8 11.4 9 Vehicle N/A IV 11.7 1.0 25.5 2.7 25.2 2.3 22.9 2.4 23.31.5 10 hUTC   1 × 10⁶ IV 11.9 1.1 28.1 2.3 33.9 2.3

3.0

3.4 Mean ± standard errors (sem) for the measurements for specific days(post-injury) are shown. Bold and italicized numbers indicatestatistical significance compared to control.

There was no clear difference in the magnitude of effects with the 3different delivery modalities. Using 1×10⁶ hUTC in fibrin resulted inapproximately 43.4% relative perfusion at 28 days post-injury while hUTCalone resulted in a maximum relative perfusion of 40.6% (see FIG. 8).For cells delivered systemically, relative perfusion in the ischemiclimbs of mice receiving hUTC was significantly greater than the controlon days 21 and 28 post-injury (P<0.01).

Two doses of cells were tested using local (IM) administration. Thehigher dose was significantly different (P<0.05) than the control at 21and 28 days post-injury. The low dose group was not significantlydifferent than control at any day. The high and low dose groups were notsignificantly different from each other at any time point (Table 6-2).

Four different doses of hUTC in fibrin glue were tested using local (IM)administration. In the group receiving 1×10⁶ cells, relative perfusionin the ischemic limb was significantly greater than the control on days21 (P<0.05) and 28 (P<0.01) post-injury. Relative perfusion in thegroups receiving doses of 0.5, 0.25 and 0.125×10⁶ cells were allsignificantly greater than the control only at day 21 (P<0.001, P<0.01and P<0.05, respectively) post-injury. There was no difference betweenany of the dose groups (FIG. 9).

There was a slight trend toward greater reperfusion with increasingdose, which is especially apparent at 14 days post-injury (data withouterror bars shown for clarity in FIG. 10).

In summary, animals treated with hUTC delivered by all three methodsshowed increased reperfusion of ischemic limbs. In this study, there wasno clear difference in the magnitude of effects with delivery modality.It is notable that the relative perfusion was significantly higher at 28days post-injury for the highest dose groups; independent of deliveryroute or cell number.

EXAMPLE 7 Evaluation of the Efficacy of hUTC Cell Transplantation in aMouse Model of Peripheral Limb Ischemia: A Route of Administration Study

The purpose of this study was to evaluate if hUTC cell delivery restoresblood flow in a mouse model of peripheral limb ischemia (unilateralhindlimb ischemia model). A comparison was made between two routes ofadministration—intravenous and intramuscular delivery; the latter whichalso included suspension of cells in a fibrin matrix.

Methods

The treatment groups are shown in Table 7-1 below:

TABLE 7-1 Treatment Groups # of Grp # Test Animal Animals Test MaterialROA Cell Dose 1 Nude 12 Saline IV N/A 2 Nude 12 hUTC IV 1 × 10⁶ 3 Nude12 Saline IM N/A 4 Nude 12 Saline + hUTC IM 1 × 10⁶ 5 Nude 12 Saline +Fibrin IM N/A 6 Nude 12 Saline + Fibrin + IM 1 × 10⁶ hUTC

The fibrin glue formations for Groups 5 and 6, IM administration areshown below in Table 7-2:

TABLE 7-2 Fibrin glue formations for Groups 5 and 6, IM administrationGroup 5 Group 6 Cells None 1 × 10⁶ Saline (PBS)  0.075 ml  0.075 mlSolution A (thrombin) 0.0125 ml 0.0125 ml Solution B (fibrinogen) 0.0125ml 0.0125 ml All amounts shown are per animal (0.1 ml per animal)Thrombin = 1:5000 final dilution of stock solution (stock solutioncontains 1.6 μl thrombin (800-1200 IU/ml)) + 998.4 μl PBS Fibrinogen =1:8 dilution (stock solution is 55-85 mg/ml)

Male immunotolerant nude mice (8 to 10 weeks old) underwentsurgically-induced unilateral hindlimb ischemia. At 1 day after surgery,blood flow in both hindlimbs was evaluated by laser Doppler perfusionimaging (LDPI). A single dose (10⁶) of hUTC cells or vehicle control wasadministered to 6 groups of mice (N=15/group) as shown in the Table 7-1.The route of administration was either IV injection of 100 μl throughthe tail vein or the same cumulative dose via 20 μl IM injection intothe upper (3 sites) and lower (2 sites) skeletal muscle in the ischemiclimb. In 2 groups receiving IM injections, a fibrin matrix was alsoincluded.

Serial LDPI was performed at 1, 3, 7, 10, 14 and 21 days; the latterbeing the last day of the study. Swim endurance was evaluated on 3 daysbefore surgery and again at 10 days after surgery. A mouse was judged toreach its limit for swim endurance when unable to rise to the surfacewithin 5 seconds of submerging. The ratio of post-ischemia swimendurance time to the average endurance before ischemia was compared.Post-mortem gastrocnemius muscle tissue samples, obtained from ischemicand normal limbs of 5 mice from each group having reached day 21 of thestudy, were processed for histological staining of capillaries(CD31/PECAM-1) and arterioles (smooth muscle a actin). Vessel densitieswere quantitated from digitized images of immuno-stained slides.

Cell engraftment and vessel densities in tissues harvested at 7 dayswere evaluated. Vessel density analysis at 7 days was deemed not usefulgiven that the separation of mean relative perfusion values for the IVcell treatment and control groups was statistically different at 21 day.Cell engraftment assays were not performed due to technical difficultieswith the methods for cell detection.

Evaluation of Blood Flow

Blood flow in mice hindlimb was evaluated using laser Doppler imagingwith a Moor LDI device. Animals were anesthetized by isofluraneinhalation and will be placed on a heating pad set at 37° C. Toestablish baseline ischemia, blood perfusion data in plantar region ofboth hindlimbs will be collected at 24 hours after creation of injury.Serial perfusion assessment was performed at days 5, 10, 15 and 20. Datawas reported as a ratio of perfusion values in the left (ischemic)versus right (non-ischemic) limbs.

Swimming Endurance Testing

Mice were also monitored for ability to swim or stay afloat in aswimming chamber. To do this, mice were trained to stay afloat in theswimming chamber. Mice were trained everyday for 3 days. At the end ofthis period, mice were assessed according to the length of time theystay afloat until fatigue, defined as the failure to rise to the surfaceof the water to breathe within 7-10s (baseline, −3 days). At day 0, micewere subjected to unilateral hindlimb injury and cells were administered24 hours post-injury. The animals were then assessed for their swimmingability/floating endurance on days 10 and 15.

Results and Analysis

Attrition of animals due to limb necrosis was low in all groups. Allattrition occurred by 1 week. The numbers of mice in each group thatwere removed from the study (shown in parentheses) were: Group 1 (2);Group 2 (1); Group 3 (2); Group 4 (2); Group 5 (1); and Group 6 (2).

Laser Doppler Perfusion Imaging

Laser Doppler perfusion data (expressed as percentage of perfusion inthe ischemic left limb compared to the non-ischemic control right limb)is shown in FIG. 11 and Table 7-3. There was enhanced relativereperfusion in the mice treated by IV infusion of hUTC cells comparedthe control which received saline by IV infusion. This effect wassignificant at days 7, 10 and 21. There was no significant differencebetween any of the other treatment groups and the appropriate controls.An unexplained maximum in relative perfusion in all control groupanimals occurred at 14 days. By 21 days, the values in the controlanimals had decreased. The relative perfusion values at day 14 of 2 micein the IV control group were excluded based on relative values whichwere greater than 100%. Even with these exclusions, there was nodifference between the IV cell group and control at this time point.

TABLE 7-3 Means ± sems for relative perfusion values Day Dose 1 3 7 1014 21 saline iv 14.41 ± 0.85  1363 ± 1.16 23.57 ± 3.39 32.07 ± 2.80 57.29 ± 6.64* 49.53 ± 2.86 cells iv 14.19 ± 2.18 16.63 ± 2.18 41.07 ±3.34 59.46 ± 5.10 59.92 ± 3.93 67.24 ± 3.18 saline im  1422 ± 1.39 16.98± 2.39 28.82 ± 3.99 33.66 ± 5.29 39.34 ± 8.14 36.21 ± 6.14 cells im12.98 ± 0.71 25.32 ± 4.33 31.13 ± 2.58 42.95 ± 2.00 46.34 ± 1.66 55.43 ±9.84 fibrin im 13.15 ± 1.01 15.16 ± 2.08 25.64 ± 2.82 35.99 ± 2.51 50.35± 3.03 44.20 ± 3.4  fibrin + cells 12.47 ± 0.70 16.34 ± 1.73 27.49 ±1.73 43.76 ± 5.84 44.73 ± 3.12 52.84 ± 3.9  im *values for 2 miceexcluded based on ischemic limb value >100% control limb

Capillary and arteriole densities in both lower limbs were determined inimmunohistologically stained thin sections harvested at 21 days. Therewas no correlation between microvascular density and perfusion. Therelative density of capillaries was not significantly different betweencontrols and treated groups (FIG. 12).

There was no difference between arteriolar densities of controls andtreated animals (FIG. 13). There was a trend toward reduced density ofarterioles in the muscles injected directly with fibrin.

The capacity of mice to swim against a laminar flow current was assessedbefore surgery and again at 10 days after surgery. The total time ofswimming was recorded before induction of ischemia each session andcompared. There was no significant difference between controls andtreatment groups in the functional assessment.

In summary, the results show that intravenous administration of hUTClead to restoration of blood flow in ischemic muscles on day 3, day 10and day 21 post-injury. In particular, intravenous administration ofhUTC 1 day after creating ischemia resulted in accelerated reperfusionof ischemic muscles and a greater level of relative perfusion at the endof the experiment (21 days). Other treatments did not have an apparentaffect by any of the measures used in this study. The mechanism by whichIV delivered hUTC enhanced reperfusion was not apparent based on theanalysis of vessel re-growth in the ischemic region. It is possible thatother mechanisms may explain the observed effects. Recently it has beenshown that systemically delivered bone marrow-derived mesenchymal stemcells trap in the lung where they promote protection at a distance viasecretion of anti-inflammatory factors which may reduce the degree ofearlier injury to the tissues (Lee et al. (2009) Stem Cell. 5(1):54-63).

The present invention is not limited to the embodiments described andexemplified above. It is capable of variation and modification withinthe scope of the appended claims.

What is claimed is:
 1. A method of improving blood flow in ischemictissue in a patient having peripheral ischemia, comprising administeringby intramuscular injection or injection into adipose depots in muscle apharmaceutical composition comprising a pharmaceutically acceptablecarrier and a mixture of fibrin and an isolated homogenous population ofcells obtained from human umbilical cord tissue in an amount effectiveto improve blood flow in the ischemic tissue, wherein the umbilical cordtissue is substantially free of blood, and wherein said isolatedhomogenous population of the cells is capable of self-renewal andexpansion in culture, has the potential to differentiate and further hasthe following characteristics: (a) expresses oxidized low densitylipoprotein receptor 1, chemokine receptor ligand 3, and granulocytechemotactic protein; (b) does not express CD117, CD31, CD34, or CD45;(c) expresses, relative to a human fibroblast, mesenchymal stem cell, oriliac crest bone marrow cell, increased levels of interleukin 8 andreticulon 1; (d) has the potential to differentiate into cells of atleast a skeletal muscle, vascular smooth muscle, pericyte or vascularendothelium phenotype; and (e) expresses CD10, CD13, CD44, CD73, andCD90.
 2. The method of claim 1, wherein the pharmaceutical compositionis administered at the sites of peripheral ischemia.
 3. The method ofclaim 1, wherein the pharmaceutical composition is administered locally.4. The method of claim 1, wherein the isolated population of cells isinduced in vitro to differentiate into a skeletal muscle, vascularmuscle, pericyte or vascular endothelium lineage prior toadministration.
 5. The method of claim 1, wherein the population ofcells is genetically engineered to produce a gene product that promotestreatment of peripheral vascular disease.
 6. The method of claim 1,wherein the composition further comprises an agent selected from thegroup consisting of an antithrombogenic agent, an immunosuppressiveagent, an immunomodulatory agent, a pro-angiogenic, an antiapoptoticagent and mixtures thereof.
 7. The method of claim 1, wherein thecomposition further comprises at least one other cell type.
 8. Themethod of claim 7, wherein the other cell type is a skeletal musclecell, a skeletal muscle progenitor cell, a vascular smooth muscle cell,a vascular smooth muscle progenitor cell, a pericyte, a vascularendothelial cell, a vascular endothelium progenitor cell or othermultipotent or pluripotent stem cell.
 9. The method of claim 1, whereinthe pharmaceutical composition exerts a trophic effect.
 10. The methodof claim 9, wherein the trophic effect is proliferation of vascularendothelial cells.
 11. The method of claim 1, wherein the pharmaceuticalcomposition induces migration of vascular endothelial cells and/orvascular endothelium progenitor cells to the sites of the peripheraldisease.
 12. The method of claim 1, wherein the pharmaceuticalcomposition induces migration of vascular smooth muscle cells and/orvascular smooth muscle progenitor cells to the sites of the peripheraldisease.
 13. The method of claim 1, wherein the pharmaceuticalcomposition induces migration of pericytes to the sites of theperipheral vascular disease.
 14. A method of improving blood flow inischemic tissue in a patient having peripheral ischemia, comprisingadministering by intramuscular injection or injection into adiposedepots in muscle a mixture of fibrin and an isolated homogenouspopulation of cells obtained from human umbilical cord tissue in anamount effective to improve blood flow in the ischemic tissue, whereinthe umbilical cord tissue is substantially free of blood, and whereinsaid isolated homogenous population of the cells is capable ofself-renewal and expansion in culture, has the potential todifferentiate and further has the following characteristics: (a)expresses oxidized low density lipoprotein receptor 1, chemokinereceptor ligand 3, and granulocyte chemotactic protein; (b) does notexpress CD117, CD31, CD34, or CD45; (c) expresses, relative to a humanfibroblast, mesenchymal stem cell, or iliac crest bone marrow cell,increased levels of interleukin 8 and reticulon 1; (d) has the potentialto differentiate into cells of at least a skeletal muscle, vascularsmooth muscle, pericyte or vascular endothelium phenotype; and (e)expresses CD10, CD13, CD44, CD73, and CD90.
 15. The method of claim 14,wherein the mixture of the population of cells and fibrin isadministered at the sites of peripheral ischemia.
 16. The method ofclaim 14, wherein the mixture of fibrin glue and the population of cellsis administered locally.
 17. The method of claim 14, wherein theisolated population of cells is induced in vitro to differentiate into askeletal muscle, vascular muscle, pericyte or vascular endotheliumlineage prior to administration.
 18. The method of claim 14, wherein thepopulation of cells is genetically engineered to produce a gene productthat promotes treatment of peripheral vascular disease.
 19. The methodof claim 14, further comprising administration of an agent selected fromthe group consisting of an antithrombogenic agent, an immunosuppressiveagent, an immunomodulatory agent, a pro-angiogenic, an antiapoptoticagent and mixtures thereof.
 20. The method of claim 14 furthercomprising administration of at least one other cell type.
 21. Themethod of claim 20, wherein the other cell type is a skeletal musclecell, a skeletal muscle progenitor cell, a vascular smooth muscle cell,a vascular smooth muscle progenitor cell, a pericyte, a vascularendothelial cell, a vascular endothelium progenitor cell or othermultipotent or pluripotent stem cell.
 22. The method of claim 14,wherein the population of cells exerts a trophic effect.
 23. The methodof claim 21, wherein the trophic effect is proliferation of vascularendothelial cells.
 24. The method of claim 14, wherein the population ofcells induces migration of vascular endothelial cells and/or vascularendothelium progenitor cells to the sites of the peripheral disease. 25.The method of claim 14, wherein the population of cells inducesmigration of vascular smooth muscle cells and/or vascular smooth muscleprogenitor cells to the sites of the peripheral disease.
 26. The methodof claim 14, wherein the population of cells induces migration ofpericytes to the sites of the peripheral vascular disease.
 27. A methodof improving blood flow in ischemic tissue in a patient havingperipheral ischemia, comprising administering by intramuscular injectionor injection into adipose depots in muscle a pharmaceutical compositioncomprising a pharmaceutically acceptable carrier and a mixture of fibringlue and an isolated homogenous population of cells obtained from humanumbilical cord tissue in an amount effective to improve blood flow inthe ischemic tissue, wherein the umbilical cord tissue is substantiallyfree of blood, wherein the fibrin glue comprises from about 16 to about24 IU/ml of thrombin and from about 39.3 to about 60.7 mg/ml offibrinogen, and wherein said isolated homogenous population of the cellsis capable of self-renewal and expansion in culture, has the potentialto differentiate and further has the following characteristics: (a)expresses oxidized low density lipoprotein receptor 1, chemokinereceptor ligand 3, and granulocyte chemotactic protein; (b) does notexpress CD117, CD31, CD34, or CD45; (c) expresses, relative to a humanfibroblast, mesenchymal stem cell, or iliac crest bone marrow cell,increased levels of interleukin 8 and reticulon 1; (d) has the potentialto differentiate into cells of at least a skeletal muscle, vascularsmooth muscle, pericyte or vascular endothelium phenotype; and (e)expresses CD10, CD13, CD44, CD73, and CD90.
 28. A method of improvingblood flow in ischemic tissue in a patient having peripheral ischemia,comprising administering by intramuscular injection or injection intoadipose depots in muscle a mixture of fibrin glue and an isolatedhomogenous population of cells obtained from human umbilical cord tissuein an amount effective to improve blood flow in the ischemic tissue,wherein the umbilical cord tissue is substantially free of blood,wherein the fibrin glue comprises from about 16 to about 24 IU/ml ofthrombin and from about 39.3 to about 60.7 mg/ml of fibrinogen, andwherein said isolated homogenous population of the cells is capable ofself-renewal and expansion in culture, has the potential todifferentiate and further has the following characteristics: (a)expresses oxidized low density lipoprotein receptor 1, chemokinereceptor ligand 3, and granulocyte chemotactic protein; (b) does notexpress CD117, CD31, CD34, or CD45; (c) expresses, relative to a humanfibroblast, mesenchymal stem cell, or iliac crest bone marrow cell,increased levels of interleukin 8 and reticulon 1; (d) has the potentialto differentiate into cells of at least a skeletal muscle, vascularsmooth muscle, pericyte or vascular endothelium phenotype; and (e)expresses CD10, CD13, CD44, CD73, and CD90.